Ethanol production using xylitol synthesis mutant of xylose-utilizing zymomonas

ABSTRACT

Production of ethanol using a strain of xylose-utilizing  Zymomonas  with a genetic modification of the glucose-fructose oxidoreductase gene was found to be improved due to greatly reduced production of xylitol, a detrimental by-product of xylose metabolism synthesized during fermentation.

CROSS REFERENCE TO RELATED APPLICATIONS

This application claims the benefit of U.S. Provisional Application No. 60/847,856, filed Sep. 28, 2006, which is incorporated in its entirety as a part hereof for all purposes.

Subject disclosed herein is disclosed in the following copending application, filed contemporaneously herewith and assigned to the same assignees as in this application: U.S. application Ser. No. 11/862,566, which is incorporated in its entirety as a part hereof for all purposes.

STATEMENT OF GOVERNMENT RIGHTS

This invention was made with United States government support under Contract Nos. 04-03-CA-70224 and DE-FC36-03GO13146 awarded by the Department of Energy. The government has certain rights in this invention.

FIELD OF INVENTION

The invention relates to the fields of microbiology and genetic engineering. More specifically, production of ethanol using a strain of xylose-utilizing Zymomonas with a genetic modification of the glucose-fructose oxidoreductase gene was found to be improved due to greatly reduced production of xylitol, a detrimental by-product of xylose metabolism synthesized during fermentation.

BACKGROUND OF INVENTION

Production of ethanol by microorganisms provides an alternative energy source to fossil fuels and is therefore an important area of current research. Zymomonas mobilis is a bacterial ethanologen that grows on glucose, fructose, and sucrose, metabolizing these sugars to CO₂ and ethanol via the Entner-Douderoff pathway. Though wild type strains cannot use xylose as a carbon source, recombinant strains of Z. mobilis that are able to grow on this sugar have been engineered (U.S. Pat. No. 5,514,583, U.S. Pat. No. 5,712,133, WO 95/28476, Feldmann et al. (1992) Appl Microbiol Biotechnol 38: 354-361, Zhang et al. (1995) Science 267:240-243). Xylose is the major pentose in hydrolyzed lignocellulosic materials, and therefore can provide an abundantly available, low cost carbon substrate for use in fermentation. Z. mobilis has been engineered for expression of four enzymes needed for xylose metabolism: 1) xylose isomerase, which catalyses the conversion of xylose to xylulose; 2) xylulokinase, which phosphorylates xylulose to form xylulose 5-phosphate; 3) transketolase; and 4) transaldolase (U.S. Pat. No. 5,514,583, U.S. Pat. No. 6,566,107; Zhang et al. (1995) Science 267:240-243). Through the combined actions of these four enzymes and the cell's normal metabolic machinery, three molecules of xylose are converted to two molecules of glucose 6-phosphate and one molecule of glyceraldehyde 3-phosphate, which are subsequently converted to ethanol and CO₂ on the glucose side of the pathway (see FIG. 1).

Though there has been success in engineering Z. mobilis strains for xylose metabolism, the strains do not grow and produce ethanol as well on xylose as on glucose. One factor that causes poor growth on xylose is the production of xylitol as a by-product of xylose metabolism (Feldmann et al. supra; Kim et al. (2000) Applied and Environmental Microbiology 66:186-193). Xylitol is phosphorylated by xylulose kinase to produce xylitol 5-phosphate, which accumulates in the cell and inhibits bacterial growth. Xylitol synthesis also reduces the yield of ethanol, since xylose-utilizing recombinant strains of Z. mobilis cannot convert xylitol to ethanol. In addition, xylitol is a potent inhibitor of xylose isomerase (Smith et al. (1991) Biochem J. 277:255-261), which catalyzes the first step of xylose utilization in the engineered xylose metabolism pathway. See FIG. 2 for a diagram showing xylitol synthesis and effects.

The physiological pathway and enzymes that are responsible for xylitol synthesis in vivo have not been determined. However, it has been demonstrated that cell-free extracts from wild type Z. mobilis are able to reduce xylose to xylitol when they are supplemented with NADPH (Feldmann et al., supra), and that this reaction is catalyzed by an NADPH-dependent aldose reductase. It has also been shown that Z. mobilis cell-free extracts are able to convert a small amount of xylose to xylitol without NADPH supplementation, and that xylitol production under these conditions increases 3- to 4-fold when purified xylose isomerase is also added to the reaction mixture (Danielson, 2001, University of Colorado Masters Thesis). Since xylose isomerase is able to convert xylose to xylulose, the clear implication of the latter experiment is that the Z. mobilis enzyme glucose-fructose oxidoreductase (GFOR) can use xylose as an electron donor and xylulose as an electron acceptor to generate xylitol as will be discussed in greater detail below. Thus, there are at least two pathways for xylitol production in Z. mobilis based on the in vitro experiments, but the extent to which they contribute to xylitol formation under physiological conditions remains to be determined.

For high-level production of ethanol, Z. mobilis is grown in high concentrations of a fermentable carbon source, which can result in osmotic shock. Osmotic shock manifests itself as a long lag period before growth commences when wild type strains are transferred to liquid media that contains >200 g/L of glucose or fructose or >360 g/L of sucrose (Loos et al. (1994) J Bacteriol 176:7688-7693). Furthermore, addition of sorbitol to the growth medium reduces the lag period when wild type strains are shifted to high concentrations of these sugars (Wiegert et al. (1996) Arch Microbiol 166:32-41, Loos et al supra).

It has also been shown that the periplasmic enzyme glucose-fructose oxidoreductase (GFOR) plays an important role in osmotic balance when wild type Z. mobilis is grown in concentrated mixtures of glucose and fructose (Loos et al. supra) or concentrated solutions of sucrose (Wiegert et al. supra, Loos et al. supra). Briefly, GFOR with its tightly bound co-factor, catalyzes the oxidation of glucose to gluconolactone and subsequent reduction of fructose to sorbitol in a classical Ping Pong Bi mechanism as shown in Diagram I. The sorbitol that is generated in the periplasmic space is transported into cells against a concentration gradient where it accumulates to high levels since it is not further metabolized. The high concentration of sorbitol inside the cells eliminates the osmotic pressure difference across the plasma membrane and restores osmotic balance.

A spontaneous mutant of wild type Z. mobilis that cannot generate sorbitol was show to produce higher levels of ethanol than wild type cells when it was grown on low concentrations of sucrose (<150 g/L), but this strain could not grow on high concentrations of sucrose (Kirk and Doelle (1993) Biotechnol. Letters 15:985-990). This mutant was subsequently shown to lack expression of glucose-fructose oxidoreductase (GFOR), which accounts for its inability to convert any of the sucrose-derived fructose to the unwanted by-product sorbitol (Wiegert et al. supra). It was also shown that growth of the sorbitol-deficient mutant in high concentrations of sucrose could be restored by adding sorbitol to the growth medium (Wiegert et al., supra). Thus GFOR plays a critical role in osmotic balance by synthesizing sorbitol when Z. mobilis is grown in concentrated mixtures of glucose and fructose or high concentrations of sucrose, which is hydrolyzed to glucose and fructose by the host cell's invertase.

CN1600850(A) discloses a non-xylose utilizing mutant strain of Z. mobilis that has an inactivated GFOR gene, and production of ethanol using this strain. The lack of sorbitol production with this strain resulted in higher levels of ethanol when glucose, fructose or sucrose was the carbon source.

The effects of reducing or eliminating glucose-fructose oxidoreductase enzyme activity in an engineered xylose-utilizing strain of Z. mobilis that is grown on a mixture of xylose and glucose (in the absence of any added sucrose or fructose) are not known.

The problem to be addressed is how to produce increased amounts of ethanol in fermentations using a xylose-utilizing Z. mobilis strain grown on xylose-containing medium. Applicants have solved the problem by determining the principle pathway for production of xylitol in vivo, and eliminating the enzyme activity that is responsible for its formation through gene inactivation, thereby creating a Z. mobilis strain that may be used for improved ethanol production.

SUMMARY OF INVENTION

The present invention relates to a process for production of ethanol using a strain of Zymomonas that has reduced production of xylitol and increased production of ethanol when grown in the presence of xylose. Applicants have discovered that xylitol production in xylose metabolizing Z. mobilis is predominantly mediated by the enzyme glucose-fructose oxidoreductase (GFOR). A genetically modified strain that does not express GFOR (a GFOR knockout mutant) was constructed and found to produce reduced amounts of xylitol when grown on xylose-containing sugar mixtures. The GFOR knockout mutant also consumed more xylose and produced higher concentrations of ethanol when grown in high sugar mixtures in the presence of sorbitol than the parent strain that expresses GFOR. In addition, the ethanol yield (the amount of ethanol produced per gram of sugar consumed) was significantly higher for the GFOR knockout strain.

Accordingly the invention provides a process for producing ethanol comprising,

a) providing a recombinant Zymomonas strain capable of utilizing xylose to produce ethanol, said strain comprising at least one genetic modification which reduces glucose-fructose oxidoreductase activity, and

b) culturing the strain of (a) in a medium comprising xylose whereby the xylose is converted to ethanol.

The process above provides improved conversion of xylose to ethanol relative to a recombinant Zymomonas strain without at least one genetic modification which reduces glucose-fructose oxidoreductase activity.

The process specifically improves one or more of the parameters rate, titer or yield, of xylose conversion to ethanol relative to a recombinant Zymomonas strain without at least one genetic modification which reduces glucose-fructose oxidoreductase activity.

In an aspect of the invention, the process described herein is improved in that strain of (a) above produces a reduced amount of xylitol, or no xylitol, as compared to Zymomonas strain without at least one genetic modification which reduces glucose-fructose oxidoreductase activity.

BRIEF DESCRIPTION OF THE FIGURES, BIOLOGICAL DEPOSITS AND SEQUENCE DESCRIPTIONS

The invention can be more fully understood from the following detailed description, the figures, and the accompanying sequence descriptions that form a part of this application.

FIG. 1 shows a diagram of the four enzymes (boxed) that have been used to engineer Z. mobilis for xylose utilization and biochemical pathways for ethanol production using xylose.

FIG. 2 shows a diagram of the first two steps of the engineered xylose pathway (boxed), xylitol synthesis, xylitol 5-phosphate formation (a toxic deadend intermediate), and inhibition of xylose isomerase by xylitol.

FIG. 3 shows the strategies for enzyme assays of transketolase (A), transaldolase (B), xylose isomerase (C), and xyulokinase (D).

FIG. 4 shows a plasmid map of pMODPgaptaltktCm.

FIG. 5 shows a plasmid map of pMODPgapxylABCm.

FIG. 6 shows a graph of xylose isomerase (XI) and xylulokinase (XK) activities in T2C, T3C, T4C, and T5C lines transformed with PgapxylAB.

FIG. 7 shows a graph of transaldolse (TAL) and transketolase (TKT) activities in T2C, T3C, T4C, and T5C lines transformed with PgapxylAB.

FIG. 8 shows a graph of % theoretical ethanol yield and % xylose utilization of selected adapted xylose-utilizing strain colonies.

FIG. 9 shows a graph of growth of adapted xylose-utilizing strains at 70 hr on RM (rich medium) with 5% xylose (RMX5%) before and after growing 50 generations in RM with 5% glucose (RMG).

FIG. 10 shows graphs of growth, glucose or xylose utilization, and ethanol and xylitol production for the selected strain, ZW658 in comparison to the control, 8b, in RM+10% glucose (RMG10%) (A, B) and RM+8% xylose (RMX8%) (C, D).

FIG. 11 shows graphs of growth, glucose and xylose utilization, and ethanol and xylitol production for the selected strain, ZW658 in comparison to the control, 8b, in RM+10% glucose and 8% xlose without acetate (A, B) or with 0.6% acetate (C, D).

FIG. 12 shows maps of plasmids made during construction of a suicide construct for insertional-inactivation of the GFOR gene, and the final product: GFORSp-9WW.

FIG. 13 shows maps of plasmids made for construction of a xylose isomerase expression plasmid: pZB188/Kan-XylA, and a diagram of the E. coli xylose isomerase expression cassette that was used for this construct (boxed).

FIG. 14 shows graphs of xylitol and xylulose production by ZW1 strains with and without GFOR gene inactivation, in the presence and absence of xylose isomerase expression.

FIG. 15 shows graphs of growth, glucose and xylose utilization, and ethanol production of xylose-utilizing Z. mobilis strains without (A) and with (B) GFOR gene inactivation, grown on 97 g/L total xylose+glucose.

FIG. 16 shows graphs of growth, glucose and xylose utilization, and ethanol production of xylose-utilizing Z. mobilis strains without (A) and with (B) GFOR gene inactivation, grown on 188 g/L total xylose+glucose.

FIG. 17 shows a graph of growth of a xylose-utilizing Z. mobilis strain with GFOR gene inactivation in the presence of different concentrations of sorbitol.

FIG. 18 shows graphs of xylose utilization, ethanol production, and xylitol production of xylose-utilizing Z. mobilis strains without (A, C) and with (B, D) GFOR gene inactivation, in the absence (A, B) and presence (C, D) of acetate in 174 g/L of total xylose+glucose.

FIG. 19 shows graphs of xylose utilization, ethanol production, and xylitol production of xylose-utilizing Z. mobilis strains without (A, C) and with (B, D) GFOR gene inactivation, in the absence (A, B) and presence (C, D) of acetate in 203 g/L of total xylose+glucose.

FIG. 20 shows graphs of xylose utilization, ethanol production, and xylitol production of xylose-utilizing Z. mobilis strains without (A, C) and with (B, D) GFOR gene inactivation, in the absence (A, B) and presence (C, D) of acetate in 203 g/L of total xylose+glucose with additional potassium bicarbarbonate for increased buffering capacity.

FIG. 21 shows a graph of xylose and glucose utilization, ethanol production, and xylitol production of a xylose-utilizing Z. mobilis strain with GFOR gene inactivation, in the presence of acetate in 189 g/L of total xylose+glucose in a pH-controlled fermentation run.

FIG. 22 shows plasmid maps of pZB188/Kan and pZB188/kan-Cre, a Cre Expression vector that can replicate in Z. mobilis.

FIG. 23A shows a comparison of the growth of ZW801-4 and ZW800 in high glucose+xylose, with acetate under pH-controlled conditions. FIG. 23B shows a graph of, glucose and xylose utilization, and ethanol production for ZW801-4 in comparison to ZW800.

FIG. 24 shows an alignment of the translated mutant sequence in ZW801-4 with the wild type GFOR protein. The wild type GFOR sequence (labeled as 39; SEQ ID NO:39) is the bottom line. The mutant sequence encodes two amino acid sequences (labeled as 40 and 41; SEQ ID NOs:40 and 41) that are separated by a stop codon (*) in the top line.

The invention can be more fully understood from the following detailed description and the accompanying sequence descriptions which form a part of this application.

The following sequences conform with 37C.F.R. 1.821-1.825 (“Requirements for Patent Applications Containing Nucleotide Sequences and/or Amino Acid Sequence Disclosures—the Sequence Rules”) and consistent with World Intellectual Property Organization (WIPO) Standard ST.25 (1998) and the sequence listing requirements of the EPO and PCT (Rules 5.2 and 49.5(a-bis), and Section 208 and Annex C of the Administrative Instructions). The symbols and format used for nucleotide and amino acid sequence data comply with the rules set forth in 37 C.F.R. §1.822.

A Sequence Listing is provided herewith on Compact Disk. The contents of the Compact Disk containing the Sequence Listing are hereby incorporated by reference in compliance with 37 CFR 1.52(e). The Compact Discs are submitted in duplicate and are identical to one another. The discs are labeled “Copy 1—Sequence Listing” and “Copy 2 Sequence listing” The discs contain the following file: CL3662 seq list.ST25.

SEQ ID NOs:1 and 2 are the nucleotide sequences of primers for amplification of a DNA fragment containing the glyceraldehyde-3-phosphate dehydrogenase gene promoter (P_(gap)) from pZB4.

SEQ ID NOs:3 and 4 are the nucleotide sequences of primers for amplification of a DNA fragment containing a tal coding region from pZB4.

SEQ ID NOs:5 and 6 are the nucleotide sequences of primers for amplification of a DNA fragment containing P_(gap)tal from the P_(gap) and tal fragments.

SEQ ID NOs:7 and 8 are the nucleotide sequences of primers for amplification of a DNA fragment containing loxP::Cm from pZB186.

SEQ ID NO:9 is the complete nucleotide sequence for the pMODP_(gap)taltktCm plasmid.

SEQ ID NOs:10 and 11 are the nucleotide sequences of primers for amplification of a 3 kb DNA fragment containing tal and tkt coding regions in transformants receiving pMODP_(gap)taltktCm.

SEQ ID NO:12 is the complete nucleotide sequence for the pMODP_(gap)xylABCm plasmid.

SEQ ID NOs:13 and 14 are the nucleotide sequences of primers for amplification of a 1.6 kb P_(gap)xylA DNA fragment from the T2C, T3C, T4C and T5C integrants with pMODP_(gap)xylABCm.

SEQ ID NOs:15 and 16 are the nucleotide sequences of primers for amplification of a 1.3 kb xylB DNA fragment from the T2C, T3C, T4C and T5C integrants with pMODP_(gap)xylABCm.

SEQ ID NOs:17 and 18 are the nucleotide sequences of primers for amplification of a 2268 bp DNA frag from Z. mobilis W1 genomic DNA containing a portion of the 3′ end of the pgm gene, the Idh gene, and a portion of the 5′ end of the adhI gene.

SEQ ID NOs:19 and 20 are the nucleotide sequences of primers for amplification of the tetracycline resistance cassette from pACYC184.

SEQ ID NOs:21 and 22 are oligonucleotide sequences used to create a loxP site.

SEQ ID NOs:23 and 24 are oligonucleotide sequences used to create a loxP site.

SEQ ID NOs:25 and 26 are the nucleotide sequences of primers for amplification of the Spec^(r)-cassette from pHP15578.

SEQ ID NOs:27 and 28 are the nucleotide sequences of primers for amplification of 3′ GFOR flanking DNA from ZW1 genomic DNA.

SEQ ID NOs:29 and 30 are the nucleotide sequences of primers for amplification of 5′ GFOR flanking DNA from ZW1 genomic DNA.

SEQ ID NO:31 is the nucleotide sequence of the pGFORSp-9WW plasmid.

SEQ ID NOs:32 and 33 are the nucleotide sequences of primers for amplification of the Kan^(r)-cassette from pET-24a.

SEQ ID NO:34 is the nucleotide sequence of the E. coli xylA expression cassette that was derived from pZB4.

SEQ ID NOs:35 and 36 are the nucleotide sequences of primers for amplification of a Cre-expression cassette.

SEQ ID NO:37 is the complete nucleotide sequence of the disrupted GFOR coding region in ZW801-4 (from the original start codon through the original stop codon), SEQ ID NO:38 is the complete nucleotide sequence of the wild type GFOR coding region (from the original start codon through the original stop codon),

SEQ ID NO:39 is the amino acid sequence encoded by SEQ ID NO:38.

SEQ ID NO:40 is the amino acid sequence encoded by the 5′ portion of SEQ ID NO:37 up to the internal stop codon.

SEQ ID NO:41 is the amino acid sequence encoded by the 3′ portion of SEQ ID NO:37 following the internal stop codon.

Applicants made the following biological deposit under the terms of the Budapest Treaty on the International Recognition of the Deposit of Micro-organisms for the Purposes of Patent Procedure at the American Type Culture Collection (ATCC) 10801 University Boulevard, Manassas, Va. 20110-2209:

Depositor Identification International Depository Date of Reference Designation Deposit ZW658 ATCC # PTA-7858 Sep. 12, 2006

DETAILED DESCRIPTION

The present invention describes a process for producing ethanol from fermentation using genetically modified xylose-utilizing Zymomonas strains with reduced GFOR enzyme activity. The xylose-utilizing recombinant Zymomonas used in the processes further engineered with at least one modification in the glucose-fructose oxidoreductase (GFOR) gene such that expression of the active enzyme is reduced or eliminated. Applicants show that elimination of GFOR enzyme activity results in reduced xylitol production during xylose metabolism and enhanced ethanol production. Ethanol produced by the new Zymomonas strain may be used as an alternative energy source to fossil fuels.

The following abbreviations and definitions will be used for the interpretation of the specification and the claims.

“Glucose-fructose oxidoreductase” is abbreviated GFOR.

RM is rich medium.

RMG5% is RM+5% glucose.

RMG10% is RM+10% glucose.

RMX8% is RM+8% xylose.

RMX2% is RM+2% xylose.

RMX5% is RM+5% xylose.

RMGX10%8% is RM+10% glucose and 8% xylose.

RMGX5%8% is RM+5% glucose and 8% xylose.

“Gene” refers to a nucleic acid fragment that expresses a specific protein, including regulatory sequences preceding (5′ non-coding sequences) and following (3′ non-coding sequences) the coding sequence. “Native gene” or “wild type gene” refers to a gene as found in nature with its own regulatory sequences. “Chimeric gene” refers to any gene that is not a native gene, comprising regulatory and coding sequences that are not found together in nature. Accordingly, a chimeric gene may comprise regulatory sequences and coding sequences that are derived from different sources, or regulatory sequences and coding sequences derived from the same source, but arranged in a manner different than that found in nature. “Endogenous gene” refers to a native gene in its natural location in the genome of an organism. A “foreign” gene refers to a gene not normally found in the host organism, but that is introduced into the host organism by gene transfer. Foreign genes can comprise native genes inserted into a non-native organism, or chimeric genes.

The term “genetic construct” refers to a nucleic acid fragment that encodes for expression of one or more specific proteins. In the gene construct the gene may be native, chimeric, or foreign in nature. Typically a genetic construct will comprise a “coding sequence”. A “coding sequence” refers to a DNA sequence that codes for a specific amino acid sequence.

“Promoter” or “Initiation control regions” refers to a DNA sequence capable of controlling the expression of a coding sequence or functional RNA. In general, a coding sequence is located 3′ to a promoter sequence. Promoters may be derived in their entirety from a native gene, or be composed of different elements derived from different promoters found in nature, or even comprise synthetic DNA segments. It is understood by those skilled in the art that different promoters may direct the expression of a gene in different tissues or cell types, or at different stages of development, or in response to different environmental conditions. Promoters which cause a gene to be expressed in most cell types at most times are commonly referred to as “constitutive promoters”.

The term “expression”, as used herein, refers to the transcription and stable accumulation of sense (mRNA) or antisense RNA derived from a gene. Expression may also refer to translation of mRNA into a polypeptide. “Antisense inhibition” refers to the production of antisense RNA transcripts capable of suppressing the expression of the target protein. “Overexpression” refers to the production of a gene product in transgenic organisms that exceeds levels of production in normal or non-transformed organisms. “Co-suppression” refers to the production of sense RNA transcripts capable of suppressing the expression of identical or substantially similar foreign or endogenous genes (U.S. Pat. No. 5,231,020).

The term “Messenger RNA (mRNA)” as used herein, refers to the RNA that is without introns and that can be translated into protein by the cell.

The term “non-functional gene” as used herein refers to a gene that does not express the encoded protein normally as in the wild type strain where the gene is endogenous. Expression of a non-functional gene may be disrupted at any level, such as transcription, RNA processing, or translation. A non-functional gene typically has little or no expression of the encoded protein. However it may also code for a modified protein that has lower enzyme activity than the wild type protein.

The term “transformation” as used herein, refers to the transfer of a nucleic acid fragment into a host organism, resulting in genetically stable inheritance. The transferred nucleic acid may be in the form of a plasmid maintained in the host cell, or some transferred nucleic acid may be integrated into the genome of the host cell. Host organisms containing the transformed nucleic acid fragments are referred to as “transgenic” or “recombinant” or “transformed” organisms.

The terms “plasmid” and “vector” as used herein, refer to an extra chromosomal element often carrying genes which are not part of the central metabolism of the cell, and usually in the form of circular double-stranded DNA molecules. Such elements may be autonomously replicating sequences, genome integrating sequences, phage or nucleotide sequences, linear or circular, of a single- or double-stranded DNA or RNA, derived from any source, in which a number of nucleotide sequences have been joined or recombined into a unique construction which is capable of introducing a promoter fragment and DNA sequence for a selected gene product along with appropriate 3′ untranslated sequence into a cell.

The term “operably linked” refers to the association of nucleic acid sequences on a single nucleic acid fragment so that the function of one is affected by the other. For example, a promoter is operably linked with a coding sequence when it is capable of affecting the expression of that coding sequence (i.e., that the coding sequence is under the transcriptional control of the promoter). Coding sequences can be operably linked to regulatory sequences in sense or antisense orientation.

The term “selectable marker” means an identifying factor, usually an antibiotic or chemical resistance gene, that is able to be selected for based upon the marker gene's effect, i.e., resistance to an antibiotic, wherein the effect is used to track the inheritance of a nucleic acid of interest and/or to identify a cell or organism that has inherited the nucleic acid of interest.

The terms “substantially eliminated” xylitol production and “substantially no” by-product xylitol refer to the case where the amount of xylitol detected using typical laboratory analysis is close to zero.

The term “high concentration of mixed sugars” refers to a total sugar concentration in the medium that results in inhibition of growth of GFOR mutant xylose-utilizing Z. mobilis. This is typically greater than about 100 g/L, although the exact concentration may vary depending on other components in the medium.

The term “fermentable sugar” refers to oligosaccharides and monosaccharides that can be used as a carbon source by a microorganism in a fermentation process.

The term “lignocellulosic” refers to a composition comprising both lignin and cellulose. Lignocellulosic material may also comprise hemicellulose.

The term “cellulosic” refers to a composition comprising cellulose and additional components, including hemicellulose.

The term “saccharification” refers to the production of fermentable sugars from polysaccharides.

The term “pretreated biomass” means biomass that has been subjected to pretreatment prior to saccharification.

“Biomass” refers to any cellulosic or lignocellulosic material and includes materials comprising cellulose, and optionally further comprising hemicellulose, lignin, starch, oligosaccharides and/or monosaccharides. Biomass may also comprise additional components, such as protein and/or lipid. Biomass may be derived from a single source, or biomass can comprise a mixture derived from more than one source; for example, biomass could comprise a mixture of corn cobs and corn stover, or a mixture of grass and leaves. Biomass includes, but is not limited to, bioenergy crops, agricultural residues, municipal solid waste, industrial solid waste, sludge from paper manufacture, yard waste, wood and forestry waste. Examples of biomass include, but are not limited to, corn grain, corn cobs, crop residues such as corn husks, corn stover, grasses, wheat, wheat straw, barley, barley straw, hay, rice straw, switchgrass, waste paper, sugar cane bagasse, sorghum, soy, components obtained from milling of grains, trees, branches, roots, leaves, wood chips, sawdust, shrubs and bushes, vegetables, fruits, flowers and animal manure.

“Biomass hydrolysate” refers to the product resulting from saccharification of biomass. The biomass may also be pretreated prior to saccharification.

Standard recombinant DNA and molecular cloning techniques used here are well known in the art and are described by Sambrook, J., Fritsch, E. F. and Maniatis, T. Molecular Cloning: A Laboratory Manual, 2^(nd) ed.; Cold Spring Harbor Laboratory: Cold Spring Harbor, N.Y., 1989 (hereinafter “Maniatis”); and by Silhavy, T. J., Bennan, M. L. and Enquist, L. W. Experiments with Gene Fusions; Cold Spring Harbor Laboratory: Cold Spring Harbor, N.Y., 1984; and by Ausubel, F. M. et al., In Current Protocols in Molecular Biology, published by Greene Publishing and Wiley-Interscience, 1987.

The present invention relates to a process for producing ethanol from xylose-containing medium using GFOR mutants of xylose-utilizing Zymomonas. The engineered strains of xylose-utilizing Zymomonas with reduced GFOR enzyme activity have enhanced ethanol production. A challenge for improving ethanol production by xylose-utilizing Z mobilis is reducing or eliminating the synthesis of xylitol, which (a) represents a non-value adding carbon sink; (b) inhibits the first step of xylose utilization; and (c) is phosphorylated to a toxic deadend intermediate that inhibits bacterial growth. Applicants have discovered that the endogenous enzyme GFOR is predominantly responsible for xylitol synthesis in vivo and that by reducing or eliminating GFOR enzyme activity, ethanol production (rate, yield and titer) from xylose is improved.

Xylose-Utilizing Zymomonas Host Strain

Any strain of Zymomonas that is able to utilize xylose as a carbon source may be used as a host for preparing the strains used in the present process. Strains of Z. mobilis that have been engineered for xylose fermentation to ethanol are particularly useful. Endogenous genes may provide part of the metabolic pathway, or may be altered by any known genetic manipulation technique to provide a protein with enzyme activity useful for xylose metabolism. For example, the endogenous transketolase may complement other introduced enzyme activities in creating a xylose utilization pathway. Typically four genes have been introduced into Z mobilis for expression of four enzymes involved in xylose metabolism (FIG. 1) as described in U.S. Pat. No. 5,514,583, which is herein incorporated by reference. These include genes encoding xylose isomerase, which catalyzes the conversion of xylose to xylulose and xylulokinase, which phosphorylates xylulose to form xylulose 5-phosphate. In addition, transketolase and transaldolase, two enzymes of the pentose phosphate pathway, convert xylulose 5-phosphate to intermediates that couple pentose metabolism to the glycolytic Entner-Douderoff pathway permitting the metabolism of xylose to ethanol. DNA sequences encoding these enzymes may be obtained from any of numerous microorganisms that are able to metabolize xylose, such as enteric bacteria, and some yeasts and fungi. Sources for the coding regions include Xanthomonas, Klebsiella, Escherichia, Rhodobacter, Flavobacterium, Acetobacter, Gluconobacter, Rhizobium, Agrobacterium, Salmonella, Pseudomonads, and Zymomonas. Particularly useful are the coding regions of E. coli.

The encoding DNA sequences are operably linked to promoters that are expressed in Z. mobilis cells such as the promoters of Z. mobilis glyceraldehyde-3-phosphate dehydrogenase (GAP promoter), and Z. mobilis enolase (ENO promoter). The coding regions may individually be expressed from promoters, or two or more coding regions may be joined in an operon with expression from the same promoter. The resulting chimeric genes may be introduced into Zymomonas and maintained on a plasmid, or integrated into the genome using, for example, homologous recombination, site-directed integration, or random integration. Xylose-utilizing strains that are of particular use include CP4(pZB5) (U.S. Pat. No. 5,514,583), ATCC31821/pZB5 (U.S. Pat. No. 6,566,107), 8b (US 20030162271; Mohagheghi et al., (2004) Biotechnol. Lett. 25; 321-325), and ZW658 (described herein; deposited, ATTCC # PTA-7858).

Zymomonas strains that are additionally engineered to utilize sugars other than xylose, which it does not naturally use, may be used in the present process. An example is a strain of Z. mobilis engineered for arabinose utilization as described in U.S. Pat. No. 5,843,760, which is herein incorporated by reference.

Discovery of Xylitol Synthesis by GFOR

Synthesis of the unwanted by-product xylitol by xylose-utilizing strains of Z. mobilis reduces the yield of ethanol and results in the formation of xylitol 5-phosphate which is a toxic compound that inhibits bacterial growth (see FIG. 2). In addition, xylitol is a potent inhibitor of xylose isomerase, the first enzyme in the engineered pathway for xylose utilization, and its synthesis reduces the ability of the cells to metabolize xylose. Although in vitro experiments have established that there are at least two pathways for xylitol formation in Z. mobilis (Feldmann et al. supra, Danielson et al. supra), applicants have discovered that the majority of xylitol that is produced physiologically is the result of GFOR enzyme activity. Applicants have found that the amount of xylitol that is synthesized by Z. mobilis strains that can utilize xylose (or xylulose synthesizing derivatives of wild type Z. mobilis) that are grown on xylose-containing media is greatly reduced in the absence of GFOR enzyme activity. Applicants also found that conversion of xylose to xylulose is a prerequisite for GFOR-mediated xylitol production in vivo, and that this reaction can only occur in Z. mobilis strains that express xylose isomerase. Thus it is proposed that the major physiological source of xylitol in Z. mobilis strains that are engineered to grow on xylose is synthesized by GFOR via one or both of the reactions that are depicted in Diagrams II and III.

Note that in both schemes xylulose serves as the obligatory electron acceptor for GFOR and that this compound is reduced to xylitol in contrast to the known reaction with fructose that results in sorbitol production (Diagram I). Although GFOR is quite specific for glucose and fructose, it has been shown that it can use other sugars as electron donors and electron acceptors, albeit rather poorly (Zachariou and Scopes (1986) Journal of Bacteriology 167:863-869). Thus, when xylose and fructose were incubated with the purified protein, sorbitol production was observed but there was about a 12-fold reduction in GFOR enzyme activity compared to the control reaction with glucose. In the same paper it was shown that xylulose can substitute for fructose as an electron acceptor, and that this reaction gives rise to xylitol as depicted in Diagram III. However, with this combination of substrates there was about a 14-fold decrease in GFOR enzyme activity. In addition to these observations, it has also been shown that cell-free extracts prepared from wildtype Z. mobilis are able to generate xylitol from xylose when purified xylose isomerase is added to the reaction mixture to provide a source of xylulose (Danielson supra), thus demonstrating that GFOR can also catalyze the reaction that is depicted in Diagram II. However, whether or not these GFOR-mediated reactions occur in living cells and, if they do, to what extent they contribute to xylitol formation in vivo remained to be determined prior to applicants' discovery. The same uncertainties pertained to the NADPH-dependent aldose reductase activity that is also present in wild type Z. mobilis cell-free extracts, that is able to directly convert xylose to xylitol (Feldmann et al. supra). Indeed, none of the experiments with cell-free extracts noted above provided any insight on the relative contributions of GFOR and NADPH-dependent aldose reducatase to xylitol formation in vitro, let alone in vivo under process relevant conditions. Thus applicants' finding that GFOR is principally responsible for xylitol production in Z. mobilis strains that are engineered to grow on xylose under physiological conditions in xylose containing media was surprising and could not be anticipated from prior art.

Altering GFOR Gene Expression

A xylose-utilizing Zymomonas strain used in the present process is engineered such that there is reduced or no expression of the GFOR encoding gene, so that xylitol synthesis is reduced. Any genetic modification method known by one skilled in the art for reducing the presence of a functional enzyme may be used to alter GFOR expression. Methods include, but are not limited to, deletion of the entire gene or a portion of the gene encoding GFOR, inserting a DNA fragment into the GFOR gene (in either the promoter or coding region) so that the protein is not expressed or is expressed at lower levels, introducing a mutation into the GFOR coding region which adds a stop codon or frame shift such that a functional protein is not expressed, and introducing one or more mutations into the GFOR coding region to alter amino acids so that a non-functional or a less enzymatically active protein is expressed. In addition, GFOR expression may be blocked by expression of an antisense RNA or an interfering RNA, and constructs may be introduced that result in cosuppression. All of these methods may be readily practiced by one skilled in the art making use of the known sequence encoding GFOR (SEQ ID NO:38). DNA sequences surrounding the GFOR coding sequence are also useful in some modification procedures and are available for Z. mobilis in the complete genome sequence (GenBank Accession #AE008692).

A particularly suitable method for creating a genetically modified GFOR strain, as exemplified herein in Examples 3 and 5, is using homologous recombination mediated by GFOR flanking DNA sequences bounding a spectinomycin resistance gene or other selectable marker, leading to insertion of the selectable marker in the GFOR coding region such that a functional GFOR enzyme is not expressed. In addition, the selectable marker may be bounded by site-specific recombination sites, so that following expression of the corresponding site-specific recombinase, the resistance gene is excised from the GFOR gene without reactivating the latter. The site-specific recombination leaves behind a recombination site which disrupts expression of the GFOR enzyme. The homologous recombination vector may be constructed to also leave a deletion in the GFOR gene following excision of the selectable marker, as is well known to one skilled in the art.

It is preferred to completely eliminate the expression of GFOR, however use of recombinant Zymomonas strains with greatly reduced expression of GFOR is also an embodiment of the present process. In this case, a non-functional GFOR gene refers to not functioning in the normal manner such that lower than normal levels of GFOR enzyme are present. Some methods of gene inactivation may result in some remaining low-level expression, such as co-suppression. Herein, a modified GFOR strain refers to a genetically modified strain with reduced or no GFOR enzyme activity.

Growth and Ethanol Production by GFOR Modified Strain

A GFOR modified xylose-utilizing Zymomonas strain used in the present process is grown in a medium containing xylose in the absence or presence of other sugars (“mixed sugars”). The mixed sugars include at least one additional sugar to xylose. Any sugar that may provide an energy source for metabolism of the Zymomonas cells, or any sugar that is present in a mixture containing xylose may be included. It is desirable to grow GFOR modified xylose-utilizing Z. mobilis cells on sugars that are produced from biomass saccharification. Typically biomass is pretreated, for example as described in Patent Application WO2004/081185 and in co-owned and co-pending U.S. application Ser. No. 11/402,757, and then treated with saccharification enzymes as reviewed in Lynd, L. R., et al. (Microbiol. Mol. Biol. Rev. (2002) 66:506-577). Biomass saccharification produces sugars that may typically include a mixture of xylose with glucose, fructose, sucrose, galactose, mannose, and/or arabinose. Preferred is a mixed sugars composition that includes xylose and glucose, where additional sugars may be present.

The ratio of different sugars may vary in the mixture, with xylose typically at least about 10% of the total amount of sugars. Preferably xylose is between about 40% and about 60%. Fructose is present in sugars produced by saccharification of some biomass such as sugar cane bagasse, and may replace a portion of xylose or glucose, such that xylose remains at least about 10% of the sugar mixture. In addition, arabinose is derived from hemicellulose and thus is a typical component of mixed sugars derived from saccharified biomass containing hemicellulose.

Under fermentation conditions where xylitol would not be produced by a xylose-utilizing Z. mobilis strain that is not a GFOR modified strain, GFOR modified xylose-utilizing Z. mobilis strains grow and produce ethanol comparably to non-GFOR modified strains. For example, in low sugar medium, such as at about 100 g/L mixed sugars with a 5:4 ratio of glucose to xylose, the GFOR modified xylose-utilizing Z. mobilis cells perform similarly to non-GFOR modified strains.

For maximal ethanol production and efficiency of fermentation it is desirable to grow a xylose-utilizing ethanologen in medium containing high levels of sugars, including xylose. The mixed sugars may be used in a high concentration in medium for growth of GFOR modified xylose-utilizing Z. mobilis strains in the present process. This allows the direct use of biomass saccharification sugars, or use with little dilution, thereby reducing fermentation volumes, which is desirable for commercial scale ethanol production. High sugars concentrations are used so that greater concentrations of ethanol may be produced. The mixed sugars concentration in the fermentation medium is typically at least about 120 g/L and up to about 300 g/L. Particularly useful is a high concentration of mixed sugars that is between about 150 g/L and about 235 g/L.

In the high concentration mixed sugars conditions desired for production of ethanol, sorbitol is included in the fermentation medium for the GFOR modified xylose-utilizing Z. mobilis. Applicants surprisingly found that addition of sorbitol to the high mixed sugars medium allowed good growth of GFOR modified xylose-utilizing Z. mobilis, whereas without inclusion of sorbitol the GFOR modified xylose-utilizing Z. mobilis showed little or no growth. This is in marked contrast to GFOR producing strains that are able to adapt to the concentrated sugar mixture without sorbitol addition after a 12-36 hour lag period. In medium lacking fructose or sucrose (as a source of fructose), it was not expected that GFOR would synthesize sorbitol or play a role in osmotic adaptation. With no fructose present in the growth medium, the known reaction of GFOR for sorbitol synthesis, shown in Diagram I, could not proceed. The ability of xylose-utilizing Z. mobilis strains with normal GFOR enzyme activity to grow in a concentrated mixture of glucose and xylose, albeit with a long lag period, suggested that sorbitol synthesis by GFOR was not needed for osmotic adaptation, since without fructose GFOR would not be expected to synthesize sorbitol. Thus eliminating GFOR enzyme activity was not expected to have an effect on the level of sorbitol production in growth medium that lacks fructose, and a sorbitol requirement for growth of the GFOR modified xylose-utilizing Z. mobilis strain in a concentrated mixture of glucose and xylose was completely unexpected.

Sorbitol (D-sorbitol and/or L-sorbitol) may be present in the medium at concentrations that are between about 0.5 mM and 200 mM. More suitable final concentrations in the medium are concentrations between about 2 mM and 100 mM, with concentrations between 5 mM and 20 mM preferred. Mannitol may be used in the medium instead of sorbitol, or in combination with sorbitol. Mannitol was found to have similar effects to those of sorbitol in co-owned and co-pending U.S. application Ser. No. 11/862,522, which is herein incorporated by reference. In addition, it was found that galactitol and/or ribitol may be used in place of or in combination with sorbitol and/or mannitol. Sorbitol, mannitol, galactitol, ribitol or combinations thereof are all used in the same concentrations as described for sorbitol. Under fermentation conditions where xylitol would be produced by a xylose-utilizing Z. mobilis strain that is not a GFOR modified strain, such as in high sugar medium in the presence or absence of inhibitors such as acetate, GFOR modified xylose-utilizing Z. mobilis strains used in the process outperform non-GFOR modified strains. Applicants found that both the total amount of xylose that is consumed and the final ethanol titer are greater for a GFOR modified strain than a non-modified strain. Furthermore, no xylitol was produced in fermentations by GFOR modified xylose-utilizing Z. mobilis under process-relevant conditions, although small amounts could be synthesized by a non-GFOR mechanism under certain circumstances as shown in Example 6 herein.

The improvement in xylose utilization and ethanol production varies under different fermentation conditions. Under conditions where a higher level of xylitol is produced by a GFOR non-modified xylose-utilizing Z. mobilis strain, the lack of xylitol synthesis leads to a greater effect of the GFOR mutation. For example, when an inhibitor such as acetate is present in the medium, larger amounts of xylitol are produced by GFOR non-modified strains. This xylitol production is completely eliminated by the GFOR mutation allowing a greater increase in xylose utilization and ethanol production than in conditions where low amounts of xylitol would have been produced without the GFOR mutation. Since acetate is typically present in treated cellulosic biomass, reduced sensitivity to acetate is desired in an ethanologen to be grown on carbon sources derived from treated cellulosic biomass. Thus fermentation using a GFOR modified xylose-utilizing Z. mobilis strain is particularly beneficial when biomass hydrolysate is used in fermentation.

Fermentation for Ethanol Production

For production of ethanol, recombinant GFOR modified xylose-utilizing Z. mobilis is brought in contact with medium that contains mixed sugars including xylose. When the mixed sugars concentration is high such that growth is inhibited, the medium includes sorbitol, mannitol, or a mixture thereof. Galactitol or ribitol may replace or be combined with sorbitol or mannitol. The Z. mobilis grows in the medium where fermentation occurs and ethanol is produced. The fermentation is run without supplemented air, oxygen, or other gases (which may include conditions such as anaerobic, microaerobic, or microaerophilic fermentation), for at least about 24 hours, and may be run for 30 or more hours. The timing to reach maximal ethanol production is variable, depending on the fermentation conditions. Typically, if inhibitors are present in the medium, a longer fermentation period is required. The fermentations may be run at temperatures that are between about 30° C. and about 37° C., at a pH of about 4.5 to about 7.5.

In the present process GFOR modified xylose-utilizing Z. mobilis may be grown in medium containing mixed sugars including xylose in laboratory scale fermenters, and in scaled up fermentation where commercial quantities of ethanol are produced. Where commercial production of ethanol is desired, a variety of culture methodologies may be applied. For example, large-scale production from GFOR modified xylose-utilizing Z. mobilis may be produced by both batch and continuous culture methodologies. A classical batch culturing method is a closed system where the composition of the medium is set at the beginning of the culture and not subjected to artificial alterations during the culturing process. Thus, at the beginning of the culturing process the medium is inoculated with the desired organism and growth or metabolic activity is permitted to occur adding nothing to the system. Typically, however, a “batch” culture is batch with respect to the addition of carbon source and attempts are often made at controlling factors such as pH and oxygen concentration. In batch systems the metabolite and biomass compositions of the system change constantly up to the time the culture is terminated. Within batch cultures cells moderate through a static lag phase to a high growth log phase and finally to a stationary phase where growth rate is diminished or halted. If untreated, cells in the stationary phase will eventually die. Cells in log phase are often responsible for the bulk of production of end product or intermediate in some systems. Stationary or post-exponential phase production can be obtained in other systems.

A variation on the standard batch system is the Fed-Batch system. Fed-Batch culture processes are also suitable in the present process and comprise a typical batch system with the exception that the substrate is added in increments as the culture progresses. Fed-Batch systems are useful when catabolite repression is apt to inhibit the metabolism of the cells and where it is desirable to have limited amounts of substrate in the medium. Measurement of the actual substrate concentration in Fed-Batch systems is difficult and is therefore estimated on the basis of the changes of measurable factors such as pH and the partial pressure of waste gases such as CO₂. Batch and Fed-Batch culturing methods are common and well known in the art and examples may be found in Biotechnology: A Textbook of Industrial Microbiology, Crueger, Crueger, and Brock, Second Edition (1989) Sinauer Associates, Inc., Sunderland, Mass., or Deshpande, Mukund V., Appl. Biochem. Biotechnol., 36, 227, (1992), herein incorporated by reference.

Commercial production of ethanol may also be accomplished with a continuous culture. Continuous cultures are open systems where a defined culture medium is added continuously to a bioreactor and an equal amount of conditioned medium is removed simultaneously for processing. Continuous cultures generally maintain the cells at a constant high liquid phase density where cells are primarily in log phase growth. Alternatively, continuous culture may be practiced with immobilized cells where carbon and nutrients are continuously added, and valuable products, by-products or waste products are continuously removed from the cell mass. Cell immobilization may be performed using a wide range of solid supports composed of natural and/or synthetic materials as is known to one skilled in the art.

Continuous or semi-continuous culture allows for the modulation of one factor or any number of factors that affect cell growth or end product concentration. For example, one method will maintain a limiting nutrient such as the carbon source or nitrogen level at a fixed rate and allow all other parameters to moderate. In other systems a number of factors affecting growth can be altered continuously while the cell concentration, measured by medium turbidity, is kept constant. Continuous systems strive to maintain steady state growth conditions and thus the cell loss due to medium being drawn off must be balanced against the cell growth rate in the culture. Methods of modulating nutrients and growth factors for continuous culture processes as well as techniques for maximizing the rate of product formation are well known in the art of industrial microbiology and a variety of methods are detailed by Brock, supra.

Particularly suitable for ethanol production is a fermentation regime as follows. The desired GFOR modified xylose-utilizing Z. mobilis strain is grown in shake flasks in semi-complex medium at about 30° C. to about 37° C. with shaking at about 150 rpm in orbital shakers and then transferred to a 10 L seed fermentor containing similar medium. The seed culture is grown in the seed fermentor anaerobically until OD₆₀₀ is between 3 and 6, when it is transferred to the production fermentor where the fermentation parameters are optimized for ethanol production. Typical inoculum volumes transferred from the seed tank to the production tank range from about 2% to about 20% v/v. Typical fermentation medium contains minimal medium components such as potassium phosphate (1.0-10.0 g/l), ammonium sulfate (0-2.0 g/l), magnesium sulfate (0-5.0 g/l), a complex nitrogen source such as yeast extract or soy based products (0-10 g/l). A final concentration of about 5 mM sorbitol or mannitol is present in the medium. Mixed sugars including xylose and at least one additional sugar such as glucose (or sucrose), providing a carbon source, are continually added to the fermentation vessel on depletion of the initial batched carbon source (50-200 g/l) to maximize ethanol rate and titer. Carbon source feed rates are adjusted dynamically to ensure that the culture is not accumulating glucose in excess, which could lead to build up of toxic byproducts such as acetic acid. In order to maximize yield of ethanol produced from substrate utilized, biomass growth is restricted by the amount of phosphate that is either batched initially or that is fed during the course of the fermentation. The fermentation is controlled at pH 5.0-6.0 using caustic solution (such as ammonium hydroxide, potassium hydroxide, or sodium hydroxide) and either sulfuric or phosphoric acid. The temperature of the fermentor is controlled at 30° C.-35° C. In order to minimize foaming, antifoam agents (any class-silicone based, organic based etc) are added to the vessel as needed. An antibiotic, for which there is an antibiotic resistant marker in the strain, such as kanamycin, may be used optionally to minimize contamination.

Any set of conditions described above, and additionally variations in these conditions that are well known to one skilled in the art, are suitable conditions for production of ethanol by a xylose-utilizing recombinant Zymomonas strain.

EXAMPLES

The present invention is further defined in the following Examples. It should be understood that these Examples, while indicating preferred embodiments of the invention, are given by way of illustration only. From the above discussion and these Examples, one skilled in the art can ascertain the essential characteristics of this invention, and without departing from the spirit and scope thereof, can make various changes and modifications of the invention to adapt it to various uses and conditions.

General Methods

Standard recombinant DNA and molecular cloning techniques used here are well known in the art and are described by Sambrook, J., Fritsch, E. F. and Maniatis, T., Molecular Cloning: A Laboratory Manual, 2^(nd) ed., Cold Spring Harbor Laboratory: Cold Spring Harbor, N.Y. (1989) (hereinafter “Maniatis”); and by Silhavy, T. J., Bennan, M. L. and Enquist, L. W., Experiments with Gene Fusions, Cold Spring Harbor Laboratory: Cold Spring Harbor, N.Y. (1984); and by Ausubel, F. M. et al., Current Protocols in Molecular Biology, published by Greene Publishing Assoc. and Wiley-Interscience, Hoboken, N.J. (1987).

The meaning of abbreviations is as follows: “kb” means kilobase(s), “bp” means base pairs, “nt” means nucleotide(s), “hr” means hour(s), “min” means minute(s), “sec” means second(s), “d” means day(s), “L” means liter(s), “ml” means milliliter(s), “μL” means microliter(s), “μg” means microgram(s), “ng” means nanogram(s), “mM” means millimolar, “μM” means micromolar, “nm” means nanometer(s), “μmol” means micromole(s), “pmol” means picomole(s), “Cm” means chloramphenicol, “Cm^(r)” means chloramphenicol resistant, “Cm^(s)” means chloramphenicol sensitive, “Sp^(r)” means spectinomycin resistance, “Sp^(s)” means spectinomycin sensitive, “XI” is xylose isomerase, “XK” is xylulokinase, “TAL” is transaldolase, “TKT” is transketolase, “EFT” means elapsed fermentation time, “RM” means rich medium containing 10 g/L yeast extract plus 2 g/L KH₂PO₄, “MM” means mating medium containing 10 g/L yeast extract, 5 g/L tryptone, 2.5 g/L (NH₄)₂SO₄ and 0.2 g/L KH₂PO₄.

Preparation of Cell-Free Extracts of Zymomonas for Enzymatic Assays

Cells were grown in 50 ml of RM+2% glucose at 30° C. overnight to an OD₆₀₀ of 1.0-1.2. Cells were harvested by centrifugation at 4500 rpm for 10 min at 4° C. The supernatant was discarded and the cell pellet washed with 25 ml ice-cold sonication buffer. (10 mM Tris, pH 7.6, 10 mM MgCl₂), followed by centrifugation at 4500 rpm for 10 min. The pellet was resuspended in 2.0-2.5 ml sonication buffer plus 1 mM dithiothreitol. A 500 μl aliquot was centrifuged for 1 min in an eppendorf centrifuge at 4° C. Most of supernatant was discarded, leaving ˜10-20 μl behind to keep the pellet from drying out. The cells were frozen and stored at −80° C. until assayed. Prior to assay, the cells were thawed and resuspended with 500 μl of sonication buffer plus 1 mM dithiothreitol. The mix was sonicated 2× for 45 seconds at 62% duty cycle and an output control of 2 using a Branson sonifier 450, letting samples cool ˜3-5 min between sonications. Samples were centrifuged at 14,000 rpm for 60 min in a Beckman microfuge at 4° C. The supernatant was transferred to a new tube and kept at 4° C. The Pierce BCA assay was used for determining protein concentrations.

The transketolase (TKT) assay was usually performed first since this enzyme is more labile than the others. A diagram of the TKT assay is shown in FIG. 3A.

In a microplate assay, 20 μl of cell free extract was added to each well in a reaction mix, at 30° C., that included the following final concentrations of components: 0.37 mM NADP, 50 mM Tris HCl pH 7.5, 8.4 mM Mg Cl₂, 0.1 mM TPP ((thiamine pyrophosphate chloride), 0.6 mM E4P (erythrose-4-phosphate), 4 mM BHP (betahydroxypyruvate), 4 U/ml PGI (phosphoglucose isomerase), and 4 U/ml G6PD (glucose-6-phosphate dehydrogenase). The A₃₄₀ was read on a plate reader for 3-5 min. TKT activity was calculated as follows:

1 unit corresponds to the formation of 1 μmol of D-fructose 6-phosphate/min at 30° C. U (μmole/min) = slope (dA₃₄₀/min) * volume of reaction (μL)/6220/0.55 cm (moles of NADP→NADPH is 6220 A₃₄₀ per mole per L in a 1 cm cuvette) (pathlength of 200 μl per well in microplate = 0.55 cm) Specific Activity (μmole/min-mg) = μmole/min/protein concentration (mg)

The basis of the transaldolase (TAL) assay is shown in FIG. 3B. In a microplate assay, 20 μl of cell free extract was added to each well in a reaction mix, at 30° C., that included the following final concentrations of components: 0.38 mM NADH, 87 mM thiethanolamine, 17 mM EDTA, 33 mM F6P (fructose-6-phosphate), 1.2 mM E4P (erythrose-4-phosphate), 2.0 U/ml GDH (Glycerol-3-phosphate dehydrogenase), and 20 U/ml TPI (Triose phosphate isomerase). The plate was incubated for 5 min., then the A₃₄₀ was read for 3-5 min. TAL activity was calculated as follows: 1 unit corresponds to the formation of 1 μmol of D-glyceraldehyde per minute at 30° C.

U (μmole/min) = slope (dA₃₄₀/min) * volume of reaction (μL)/6220/0.55 cm (moles of NADH→NAD is 6220 A₃₄₀ per mole per L in a 1 cm cuvette) (pathlength of 200 ul per well in microplate = 0.55 cm) Specific Activity (μmole/min-mg) = μmole/min/protein The basis of the xylose isomerase (XI) assay is shown in FIG. 3C. In a microplate assay, 20 μl of cell free extract was added to each well in a reaction mix, at 30° C., that included the following final concentrations of components: 0.256 mM NADH, 50 mM xylose, 10 mM MgSO₄, 10 mM thiethanolamine, and 1 U/ml SDH (sorbitol dehydrogenase). The A₃₄₀ was read on a plate reader for 3-5 min. XI activity was calculated as follows: 1 unit of XI corresponds to the formation of 1 μmole of D-xylulose per minute at 30° C.

U (μmole/min) = slope (dA₃₄₀/min) * volume of reaction (μL)/6220/0.55 cm (moles of NADHP→NAD is 6220 A₃₄₀ per mole per L in a 1 cm cuvette) (pathlength of 200 μl per well in microplate = 0.55 cm) Specific Activity (μmole/min − mg) = μmole/min/protein concentration (mg)

The basis of the xylulokinase (XK) assay is shown in FIG. 3D. In a microplate assay, 20 μl of cell free extract was added to each well in a reaction mix, at 30° C., that included the following final concentrations of components: 0.2 mM NADH, 50 mM Tris HCl pH 7.5, 2.0 mm MgCl₂-6H₂O, 2.0 M ATP 0.2 M PEP (phosphoenolpyruvate), 8.5 mM D-xylulose, 5 U/ml PK (pyruvate kinase), and 5 U/ml LDH (lactate dehydrognase). The A₃₄₀ was read on a plate reader for 3-5 min. XI activity was calculated as follows:

1 unit corresponds to the formation of 1 μmole of D-xylulose to D-xylulose-5-phosphate per minute at 30° C. U (μmole/min) = slope (dA₃₄₀/min) * volume of reaction (μL)/6220/0.55 cm (moles of NADH→NAD is 6220 A₃₄₀ per mole per L in a 1 cm cuvette) (pathlength of 200 μl per well in microplate = 0.55 cm) Specific Activity (μmole/min-mg) = μmole/min/protein concentration (mg) HPLC Method

The analysis was done with an Agilent 1100 series HPLC and Agilent ChemStation software for LC 3D. The column was BioRad Aminex HPX-87H (HPLC Organic Analysis Column 125-0140) with BioRad Micro-Guard Cartridge Cation-H (125-0129). The operating conditions were:

Flow 0.6 mL/min Solvent 0.01N H₂SO₄ Stop Time 25 min Injection Volume 5 μl Auto Sampler Temp Control @ 10° C. or 4° C. Column Temp 55° C. Detector Refractive Index (40° C.) with External Standard Calibration Curves

Example 1 Construction of ZW658, a Xylose-Fermenting Zymomonas mobilis Strain

ZW658 was constructed by integrating two operons, P_(gap)xylAB and P_(gap)taltkt, containing four xylose-utilizing genes encoding xylose isomerase, xylulokinase, transaldolase and transketolase, into the genome of ZW1 (ATCC #31821) via sequential transposition events, and followed by adaptation on selective media containing xylose. Previously, a xylose-fermenting Zymomonas mobilis strain called 8b was constructed, as described in United States Patent Application 20030162271, by integrating the two operons P_(gap)xylAxylB and P_(eno)taltkt, along with selectable antibiotic markers, into the genome of Zymomonas mobilis 5C via a combination of homologous recombination and transposon approaches followed by adaptation and NTG mutagenesis. In the preparation of ZW658, transposition (Epicentre's EZ::Tn in vitro transposition system) was used, as opposed to site specific homologous recombination, because this approach offers the advantages of multiple choices of integration sites and relatively high insertion frequency. The four genes encoding the xylose utilization enzymes were arranged and cloned as two separate operons: P_(gap)xylAB and P_(gap)taltkt for the integration. An antibiotic resistance marker, a chloramphenicol resistance (Cm^(r)) gene flanked by two P1 phage Cre-recombinase recognition sequences (loxP), was attached to each operon for the selection of integrants. The integration of the two operons was accomplished in a two-step, sequential manner: P_(gap)taltkt followed by P_(gap)xylAB. Cm resistance selection was used in both integration events, since it was removed by expressing a Cre recombinase on a plasmid followed by curing of the plasmid after each integration. This process allowed the use of the same antibiotic marker for selection multiple times. More importantly, it allowed the removal of the antibiotic marker introduced for selection of the integration of the operons. This process eliminated the negative impact of antibiotic resistance gene(s) on the fermentation strain for commercial use.

Construction of pMODP_(gap)taltktCm for Transposition

As described in the US Patent Application 20030162271 (Example 9 therein), a 2.2 kb DNA fragment containing the transketolase (tkt) coding region from E. coli was isolated from pUCtaltkt (US Patent Application 20030162271) by BgIII/XbaI digestion and cloned in a PMOD (Epicentre Biotechnologies, Madison, Wis.) vector digested with BamHI/XbaI, resulting in pMODtkt. A PCR fragment named P_(gap)tal was generated by fusing the promoter region of the Zymomonas mobilis gap (P_(gap); glyceraldehyde-3-phosphate dehydrogenase) gene to the coding region of E. coli transaldolase (tal) as follows. A P_(gap) fragment was amplified from pZB4, the construction of which is described in U.S. Pat. No. 5,514,583 (Example 3), using primers with SEQ ID NOs:1 and 2. pZB4 contains a P_(gap)-xylA/xylB operon and a P_(ENO)-tal/tkt operon. A tal coding region fragment was amplified from pZB4 using primers with SEQ ID NOs: 3 and 4. A P_(gap)tal fragment was amplified using the P_(gap) and tal fragments as template using primers with SEQ ID NOs:5 and 6. This fragment was digested with XbaI and cloned into the plasmid pMODtkt, upstream of the tkt coding region. A loxP::Cm fragment was generated by PCR using Cmlox(F,sfi) and Cmlox(R,sfi) primers (SEQ ID NOs:7 and 8) and pZB186 as the template. pZB186 is a combination of a native Z. mobilis plasmid and pACYC184, described in U.S. Pat. No. 514,583 (Example 3) and Zhang et al. ((1995) Science 267:240-243). Finally, the loxP::Cm PCR fragment was inserted in the SfiI site of the plasmid containing P_(gap)taltkt to form the integrative plasmid pMODP_(gap)taltktCm (FIG. 4). In this plasmid, the P_(gap)taltkt loxP::Cm fragment was inserted between two mosaic ends (transposase binding sites) in the PMOD vector. The complete nucleotide sequence for the pMODP_(gap)taltktCm plasmid is given as SEQ ID NO:9.

Transposition and Transformation of pMODP_(gap)taltktCm in ZW1

Plasmid PMOD is a pUC-based vector, and therefore is a non-replicative vector in Zymomonas. Plasmid pMODP_(gap)taltktCm was treated with transposase in the presence of Mg²⁺ at room temperature for one hour and used to transform ZW1 cells by electroporation (using a BioRad Gene Pulser set at 200 ohms, 25 μF and 16 kV/cm). Electroporated cells were incubated in a mating medium (MM), which consists of 10 g/L yeast extract, 5 g/L tryptone, 2.5 g/L (NH₄)₂SO₄, 0.2 g/L K₂HPO₄) supplemented with 50 g/L glucose and 1 mM MgSO₄ for 6 hours at 30° C. The transformation mixture was plated on agar plates containing 15 g/L Bacto agar in MM supplemented with 50 g/L glucose and 120 μg/mL chloramphenicol and incubated anerobically at 30° C. The transformants were visible after about 2 days. The transformation/transposition frequency was approx. 3×10¹/μg DNA.

A total of 39 Cm^(r) transformant colonies was obtained. Twenty-one colonies were picked and further analyzed by PCR and enzymatic activity assays. PCR using primers SEQ ID NOs:10 and 11 confirmed the presence of a 3 kb DNA fragment containing tal and tkt coding regions in the transformants. Back transformation with plasmid DNA from the 21 integrant colonies generated no back transformants in E. coli suggesting the tal and tkt were integrated in the genome of ZW1. These integrants were tested for transaldolase and transketolase activities using protocols modified for microplates (General Methods). The Pierce BCA protein assay was used for the determination of protein concentrations. The transformants were grown up in RM medium containing 2% (w/v) glucose supplemented with 120 μg/ml chloramphenicol) in 50 ml conical centrifuge tubes at 30° C. The control strains 8b and ZW1 were grown up as well (RM plus 2% glucose was used for ZW1) for enzymatic assays. Cells were harvested when the OD₆₀₀ reached 1.0. Cells were washed once and resuspended in sonication buffer (10 mM Tris-HCl, pH 7.6 and 10 mM MgCl₂). Enzymatic assays were conducted as described in US Patent Application, 20030162271. Units are given as μmole/min-mg. All samples had transaldolase and transketolase activities except for one.

Southern hybridization was performed on genomic and plasmid DNA of selected integrants digested with PstI using a tkt probe. ZW1 DNA did not hybridize with the tkt probe. A common 1.5 kb band was visible in all integrant genomic DNA samples, which is the expected DNA fragment between a PstI site in tkt and a PstI site in tal. A second visible high molecular weight (6 kb or greater) band was unique between independent lines T2, T3, T4 and T5 indicating a separate genomic integration site in each line. Interestingly, both plasmid and genomic DNA of T5 hybridized with the tkt probe indicating it was likely that P_(gap)taltkt was also integrated in T5 on the native plasmid. These four strains (T2, T3, T4 and T5) were selected for further Cre treatment to remove the Cm^(r) marker.

Cre Treatment to Remove Cm^(r) Marker from Taltkt Integrants

To remove the Cm^(r) marker from the chromosome, T2, T3, T4 and T5 were transformed with pZB188/Spec-Cre. This plasmid is a derivative of the Zymomonas-E. coli shuttle vector pZB188 [Zhang et al. (1995) Science 267:240-243; U.S. Pat. No. 5,514,583] that contains an expression cassette for Cre Recombinase. pZB188/Spec-Cre is identical to the Cre Expression vector that is described In Example 10 (pZB188/Kan-Cre), except that it has a spectinomycin-resistance gene instead of a kanamycin-resistance gene. The transformants were selected on MM agar plates supplemented with 2% glucose and 200 μg/ml spectinomycin). Sp^(r) resistant colonies were picked onto RM agar plates supplemented with 2% glucose and 200 μg/ml spectinomycin and RM agar plates supplemented with 2% glucose and 120 μg/mL Cm. One hundred percent of the colonies picked were Cm^(s) indicating the high efficiency excision of Cm^(r) by Cre. Sp^(r)Cm^(s) transformants were cultured in RM plus 2% glucose at 37° C. for 2 to 5 daily transfers to cure pZB188aadACreF. At each transfer, cells were diluted and plated on RM plus 2% glucose agar plates for picking onto additional plates of the same medium with or without 200 μg/mL Sp. Sp^(s) colonies were analyzed by PCR to confirm the loss of pZB188aadACreF. The plasmid-cured descendents of the integrants were named T2C, T3C, T4C and T5C. To examine whether these transposition integrants were stable, these 4 strains were grown in RM plus 2% glucose and then transferred to 10 ml of the same medium and grown at 37° C. in duplicate test tubes. Cells were transferred daily for ten days, or approximately 100 generations. Colonies were diluted and plated onto RMG plates for colony isolation after the 1st and 10th transfers. Twelve colonies from each transfer of each strain tested positive for the presence of P_(gap)taltkt by colony PCR using 5′ P_(gap) and 3′ tkt primers (SEQ ID NOs 1 and 11). Transaldolase and transketolase activities were also measured for isolates after the 1st and 10th transfers (as described in General Methods). All 4 integrants had similar levels of both TAL and TKT activities after 100 generations on the non-selective medium, suggesting these integrants were genetically stable.

Construction of pMODP_(gap)xylABCm for Transposition

The next step was to further integrate the P_(gap)xylAB loxP::Cm operon into the ZW1::P_(gap)taltkt integrants (T2C, T3C, T4C and T5C). The integrative plasmid pMODP_(gap)xylABCm (FIG. 5) was constructed based on the plasmid pMODP_(gap)taltktCm (FIG. 4). The P_(gap)taltkt DNA fragment was removed by SacI/SfiI digestion. An adaptor fragment containing SacI, NotI, and SfiI restriction sites was introduced by ligation. A NotI fragment of P_(gap)xylAB, that was isolated from pZB4 (U.S. Pat. No. 5,514,583), was then cloned in the NotI site of the adaptor. Xylose isomerase (XI) is encoded by xylA and xylulokinase (XK) is encoded by xylB. The complete nucleotide sequence for the pMODP_(gap)xylABCm plasmid is given as SEQ ID NO: 12.

Transposition and Transformation of pMODP_(gap)xylABCm in T2C, T3C, T4C and T5C

Using a similar approach to the integration of P_(gap)taltktCm, T2C, T3C, T4C and T5C were transformed/transposed with pMODP_(gap)xylABCm (described above) treated with transposase. Six integrants (T3CCmX1, T3CCmX2, T3CCmX3, T4CCmX1, T5CCmX1, T5CCmX2) were obtained in 2 transformation/transposition experiments following Cm selection. All were confirmed for the presence of xylAB by PCR using two sets of primers: SEQ ID NOs:13, and 14, and SEQ ID NOs: 15 and 16 except for T2CcmX1 and T2CcmX6 from which no PCR fragment was detected using the primers SEQ ID NOs:13 and 14

The integrants, including the 2 PCR negative lines, were assayed for XI, XK, TAL and TKT activities (General Methods). The results shown in FIGS. 6 and 7 indicated that the six xylAB integrants T3CCmX1, T3CCmX2, T3CCmX3, T4CCmX1, T5CCmX1, and T5CCmX2 all had XI, XK, TAL and TKT activities. XI and XK activities were newly acquired as compared to the negative parental controls (FIG. 6). TAL and TKT activities were maintained as in the parental controls. All results indicated that the proteins were made and functional. Enzyme activity levels varied, with TI and XK activities similar to those of ZW1 integrants transformed/transposed with the same plasmid. The levels of activities of XI, XK, TAL and TKT were lower than those in strain 8b.

The integration of the xylAB operon was confirmed by Southern hybridization. Both genomic and plasmid DNA of the 6 lines were digested with SphI and hybridized to a digoxenin labeled xylB probe. A common band of about 3 kb, which is generated from an SphI site in xylB and another SphI site in the adjacent cloning sites on the PMOD vector, was present in all genomic DNA samples, and in addition, higher molecular weight hybridizing bands in the genomic DNA samples indicated that there were four sites of integration for the P_(gap)xylAB operon in the chromosome. T3CCmX1 and T3CCmX2 appear to have the same integration site, T3CCmX3 and T4CCmX1 may have the same integration site, and T5CCmX1 and T5CCmX2 each have a separate integration site. Digestion of the same DNA with PstI followed by Southern hybridization with the tkt probe demonstrated that each integrant had the same hybridization pattern as its respective parental strain.

Adaptation of the ZW1::P_(gap)taltktP_(gap)xylAB Cm Integrants on Xylose Media

Despite the presence of all four enzymatic activities for xylose utilization, previous observations (US Patent Application 20030162271) indicated that the integrants may not grow on xylose immediately. Growth on xylose may occur after prolonged incubation on xylose medium (either in test tubes or on plates), a process called adaptation.

The strains were adapted as follows. ZW1::P_(gap)taltktP_(gap)xylABCm integrant strains were inoculated into test tubes and plates containing RMX (containing 10 g/l yeast extract, 2 g/l KH₂PO₄, 20 g/l or 2% (w/v) xylose as well as RMGX (RM with 0.025% (w/v) glucose, 4% (w/v) xylose). The low level of glucose was used to support initial growth to increase the chance of mutation during adaptation. One of at least five attempts at adaptation on xylose in both cultures and plates was successful. After 10 days of anaerobic incubation at 30° C., 17 and 19 colonies were visible on MMGX plated with T3CCmX1 and T3CCmX2 cells, respectively. The colonies were small and looked unhealthy (transparent) on the plates. Twelve colonies (four from T3CCmX1 plating: T3CCmX11, T3CCmX12, T3CCmX13 and T3CCmX110; eight from T3CCmX2 plating: T3CCmX24, T3CCmX25, T3CCmX26, T3CCmX27, T3CCmX28, T3CCmX29, T3CCmX211 and T3CCmX212) were inoculated in RMGCm120 and transferred into 3 ml RMX for further adaptation to obtain lines that were able to grow faster on xylose.

Adaptation of integrants in test tubes containing 3 ml RMX was conducted at 30° C. OD₆₀₀ was constantly monitored in a Spectronic 601 spectrophotometer. When the growth reached mid-log phase, the cultures were transferred into fresh tubes of RMX. This process was continued for 7 transfers. The growth rates and final ODs (non-linear readings) were improved over the transfers.

At the 6^(th) transfer, the cultures were streaked out on RMX plates to isolate single colonies. Three integrants grew faster than others on RMX streaked plates: T3CCmX13, T3CCmX26 and T3CCmX27, which are referred to as X13, X26 and X27 in the tables and discussion below. To screen for the best xylose growers, four large (L1-4) and four small (S1-4) colonies each for TX13, X26 and X27 were selected and grown in RMX test tubes so that growth, sugar utilization, and ethanol production could be monitored. Colonies were grown overnight at 30° C. followed by inoculation of OD₆₀₀=0.05 into 3 ml of RMX in test tubes in duplicates. X27 grew more slowly in RMG than the other cultures and was inoculated again 6.5 hrs later. After 69 hrs (62.5 hrs for X27), samples were taken for HPLC analysis (General Methods). FIG. 8 charts the average ethanol yield (% of theoretical yield) and xylose utilization (%) for cultures at 69 hours (62.5 hr for all X27 cultures). There was no significant difference between the large and small colonies. Although the performance of X27 was better as compared to X26 on xylose, it showed slower growth on glucose. Therefore, the top performers, large colonies of X13 (X13L3) and X26 (X26L1), were chosen for further evaluation in pH-controlled fermentations. The fermentations were conducted in RMG(6% glucose), RMX(6% xylose) and RMGX(8%:4%; glucose:xylose) at 37° C. for strains X13L3 and X26L1, as well as the control strain 8b. Fermentation of glucose by X13L3 and X26L1 grown in RMG(6%) and RMGX(8%:4%) proceeded rather quickly. The fermentation of xylose in the RMGX(8%:4%) was slower for both X13L3 and X26L1 as compared to that of strain 8b. In addition, growth on RMX(6%) at 37° C. occurred after a long lag for both X13L3 and X26L1. Several isolates, X13b, X13c and X13FL, were recovered from RMX(6%) fermentations. These isolates along with the original strains X13a (an isolate of X13L3) and X26 were subjected to Cre treatment, as described previously in this Example, to remove the Cm^(r) marker from ZW1::P_(gap)taltktP_(gap)xylABCm strains. The resulting Cre treated, Cm^(r)-free integrants were named: X13aC, X13bC, X13cC, X13FLC and X26C.

Adaptation of Integrants in Xylose Medium by Serial Transfers in RMX(5%) at 37° C.

As described earlier, adaptation of the initial ZW1::P_(gap)taltktP_(gap)xylABCm strains on RMX at 30° C. greatly improved the growth of strains in these conditions. However, the adapted strains suffered a long lag during growth and fermentation in RMX(6%) at 37° C. To further improve the integrants for xylose fermentation at preferred process conditions including higher sugar concentration and temperature, the evolutionary or adaptation process was continued in RMX(5%) at 37° C. Serial transfers were conducted and the best growers were selected. Integrants used in this process included X13aC, X13bC, X13cC, X26C and X13FLC. These 5 strains were grown in RMX at 30° C. for 6 transfers before being transferred to RMX(5%) at 37° C. for another 5 to 16 transfers. During and after all the transfers cultures were streaked on RMXplates and incubated at 37° C. to isolate single colonies. Large colonies were further streaked on RMX plates and incubated at 37° C. for 3 to 4 times to purify the colonies. Final large colonies were selected for growth testing in RMX(5%) at 37° C.

Evaluation of Strains from Adaptation in RMX(5%) Medium at 37° C.

Eighteen colonies isolated after adaptation with serial transfers were tested in RMX(5%) test tubes at 37° C. initially. Twelve strains were selected for a 2nd test tube evaluation. Strain 8b was included in all the evaluations for comparison. The 18 colonies were grown up in RMG at 37° C. overnight, centrifuged and the cells were inoculated into 4 ml of RMX(5%) at 37° C., statically in test tubes for the 1^(st) evaluation. Based on the growth (OD₆₀₀, non-linear) and end point HPLC results (low residual xylose and high ethanol), 12 strains were selected for the 2^(nd) evaluation.

One of the purposes of the 2^(nd) evaluation was to test the stability of improved growth on xylose and xylose utilization capability of the strains. All 12 strains were subjected to a stability study to see whether the adapted strains were stable after being exposed to a non-selective medium in which they were serially transferred in at 37° C. for 50 generations. Cultures before and after RMG(5%) transfers were inoculated in RMX(5%) test tubes and grown at 37° C. for evaluation. The non-linear ODs were monitored by direct reading of test tubes in a Spectronic 601 spectrophotometer. The ODs at the 70^(th) hour of growth in RMX(5%) before and after 50 generations of growth in RMG are plotted in FIG. 9. The results indicated that most strains were stable after 50 generations in RMG at 37° C. The endpoint (at stationary phase) supernatants were also analyzed by HPLC for xylose and ethanol concentrations. The low residual xylose and high ethanol concentrations in these cultures supported the fact that the strain grew and fermented xylose well.

Based on the results from the above test tube evaluation (low residual xylose, high ethanol concentration and higher OD) and a subsequent microtiter plate growth screening with high concentrations of glucose and/or xylose (up to 20%) and mixtures of glucose and xylose with acetate to select better growers in high sugars and in the presence of acetate, we decided to focus on strain #26, designated as ZW658, which exhibited the best overall performance

Example 2 Fermentation Evaluation of Top Improved Xylose-Utilization Strains at 37° C.

The following example illustrates the fermentation performance of the improved xylose-utilizing Zymomonas strain ZW658 under fermentation conditions that mimic the sugar concentrations and the acetic acid level expected in a biomass hydrolysate. Strain ZW658 was inoculated into fermentors containing RM medium supplemented with 10% glucose (RMG10%), 8% xylose (RMX8%), 10% glucose+8% xylose (RMGX10%8%) and 10% glucose+8% xylose+0.6% acetic acid (RMGXAc10%8%0.6%), respectively. All fermentations were conducted in Sixfors with 300 ml media at 150 rpm, pH5.5 and 37° C. Nitrogen was purged through the media in the fermentors overnight and stopped right before inoculation. No nitrogen was purged during the fermentation. Inocula for the fermentation were prepared with RMGX(10%,4%) at 37° C. in shake flasks (150 rpm) after reviving of the working stocks in RMG5%. Strain 8b was used as a control under the same conditions. As shown in FIG. 10, ZW658 grew more slowly on RMG10% as compared to 8b (A and B), and grew at a similar rate to 8b on RMX8% (C and D). Despite the slower growth rate, FIG. 10 shows that the ethanol yield of ZW658 (93%) was similar to that of 8b at the end of fermentation in glucose medium. In RMX8% medium, the ethanol yield was higher for ZW658 (0.46 g ethanol/g sugar) as compared to 8b (0.44 g ethanol/g sugar). ZW658 produced about 4 g/1 more ethanol as compared to 8b in RMX8%. Interestingly, ZW658 did not produce any xylitol while 8b produced a low level of xylitol (0.7 g/l) at the end of the fermentation in RMX8%. Data shown in FIG. 11 shows that ZW658 performed better as compared to 8b in fermenting 10% glucose+8% xylose with (C, D) or without (A, B) acetate, indicated by more glucose and xylose consumption, less xylitol production, and more ethanol production. Most of the glucose was used and substantial residual xylose remained at the end of the fermentation for both strains in RMG10% X8%, at 37° C. and pH5.5, although ZW658 used about 8 g/1 more xylose than 8b. Xylitol production (4.9 g/l) in ZW658 in RMG10% X8% at 37° C. and pH5.5 at the end of the fermentation was significant lower than that of 8b (8.2 g/l). In the presence of acetate (6 g/l), the cell growth of both strains was reduced significantly resulting in poor fermentation performance of both glucose and xylose, although ZW658 showed slightly better fermentation performance in terms of more glucose and xylose consumption, less xylitol production and more ethanol production. Unlike in the RMX8%, both strains produced the by-product xylitol in RMG10% X8% with or without acetate, although less xylitol was produced by ZW658 as compared to 8b. The fermentation performance of the two strains is summarized in Table 1. Overall, ZW658 performed better than 8b in pure sugar fermentations. As described in Example 1, ZW658 is free of antibiotic selection markers, which is a valuable property for fermentation organisms in commercial applications.

TABLE 1 Summary of fermentation performance of ZW658 and 8b for ethanol production. Ethanol Yield Vol. Prod. Ethanol CPI g ethanol/g sugar g/l/h g/l g/g 8b (Glu) 0.47 5.15 52 21 ZW658 (Glu) 0.48 4.13 52 15 8b (Xyl) 0.44 1.66 37 24 ZW658 (Xyl) 0.46 1.83 41 23 8b (Glu Xyl) 0.43 1.80 58 52 ZW658 (Glu Xyl) 0.45 2.03 65 35 8b (Glu Xyl Ac) 0.46 0.67 48 136 ZW658 (Glu Xyl Ac) 0.47 1.04 50 90 CPI is Cell Productivity Index: g ethanol/g dry cell weight

Example 3 Preparation of a Suicide Construct for Insertional-Inactivation of the Glucose-Fructose Oxidoreductase (GFOR) Gene in ZW1 and ZW658

The suicide construct used to knockout the gene encoding glucose-fructose oxidoreductase in ZW1 and ZW658 (“GFORSp-9WW”) was derived from another suicide construct (“pLDHSp-9WW”) that was used previously to insertionally-inactivate the gene for D-lactate dehydrogenase in Z. mobilis using host-mediated, double-crossover, homologous recombination and spectinomycin resistance as a selectable marker. pLDHSp-9WW was also derived from a number of other constructs that were previously generated. The initial precursor for all of these constructs was the plasmid vector pNEB193 (NEB #N3051S; New England Biolabs). This plasmid was chosen because it can replicate in E. coli but it cannot replicate in Z. mobilis. All of the steps and intermediates that were involved in generating the GFOR knockout construct are described below in chronological order starting with plasmid pNEB193.

Construction of pLDH193

pNEB193 was double-digested with SbfI and AscI for insertion of the DNA fragment that is described below. Both restriction sites are unique and are located in the multi-cloning region of the plasmid. The SbfI/AscI-linearized pNEB193 plasmid DNA fragment was purified using Qiagen's QIAQuick Purification Kit (catalog #28104) according to the manufacturer's protocol. The DNA fragment that was cloned into pNEB193 was a 2268 bp fragment that was PCR-amplified from Z. mobilis genomic DNA, that was isolated from strain ZW1 using Qiagen's Blood & Cell Culture Maxi Kit (catalog #13362). The synthetic oligonucleotides that were used for PCR-amplification of this fragment were Primers 1 and 2:

Primer 1 (SEQ ID NO:17) CTACTCATTTcctgcaggTGGTAACTCATTGCGCGCTC Primer 2 (SEQ ID NO:18) CATCTTACTggcgcgccAAAAATCTGCGGCTGACATAC The underlined bases of Primer 1 (forward primer) hybridize to nucleotides 1262739-1262720 of GenBank accession number AE008692 at the 3′ end of the open reading frame that codes for phosphoglyceromutase (pgm), while the lower case letters correspond to an SbfI site that was added to the 5′ end of the primer. The underlined bases of Primer 2 (reverse primer) hybridize to nucleotides 1260490-1260472 of GenBank accession number AE008692, which is just upstream from the open reading frame that codes for alcohol dehydrogenase I (adhI), while the lower case letters correspond to an AscI site that was added to the 5′ end of the primer. The 2268 bp DNA fragment that was the target for PCR-amplification therefore consists of the following elements starting from the SbfI site and ending at the AscI site: (a) the 3′ end of the pgm gene, (b) the entire Idh gene that codes for D-lactate dehydrogenase, and (c) a 5′ non-translated region of the adhI gene. The PCR product was cut with SbfI and AscI, and the resulting DNA fragment was ligated into the SbfI/AscI-linearized pNEB193 vector that was described above. The ligation reaction mixture was used to transform E. Coli JM110 and the transformed cells were plated on LB medium that contained ampicillin (100 μg/ml). Ampicillin-resistant tranformants that contained plasmids with the correct size insert were initially identified by PCR using resuspended colonies (“colony PCR”) and Primers 1 and 2. Subsequent confirmation of positive clones came from restriction digestion analysis of plasmid DNA with SbfI and AscI, and DNA sequence analysis of the 2268 bp fragment that was generated by colony PCR with the ampicillin-resistant transformants. The plasmid that was selected for further manipulation is referred to below as pLDH193. Construction of pLDHTc139#7

Plasmid pLDH193 has a unique NcoI site that is located near the middle of the Idh open reading frame. This site was used to insert a DNA fragment that confers resistance to tetracycline. The tetracycline resistance cassette (Tc^(r)-cassette) that was used for this manipulation was generated by PCR using plasmid pACYC184 (GenBank accession number X06403) as a DNA template and Primers 3 and 4 as PCR primers.

Primer 3 (SEQ ID NO:19) ACTCATTTccatggCGATCGCACTATgcggccgc AATGTAGCACCTGAAG TCAGCC Primer 4 (SEQ ID NO:20) ATCTCACTccatggCCGGCCAACTAttaatt aaGAATTGATTGGCTCCAA TTCTTG The bold underlined bases of Primer 3 (forward primer) hybridize just upstream from the promoter for the tetracycline resistance gene. Primer 3 also has three restriction sites (NcoI, AsiSI, and NotI) that were added to its 5′ end. The NcoI site is in lower case letters. The AsiSI site is underlined with a thin line. The Not I site is in italicized lower case letters. The bold underlined bases of Primer 4 (reverse primer) hybridize just downstream from the stop codon for the tetracycline resistance gene, and this primer also has three restriction sites (NcoI, FseI, and PacI) that were added to its 5′ end. Similar to the labeling above, the NcoI site is in lower case letters, the FseI site is underlined with a thin line, and the PacI site is in italicized lower case letters. The 1448 bp Tc^(r)-cassette that was generated with Primers 3 and 4 was cut with NcoI and purified by preparative agarose gel electrophoresis. The resulting DNA fragment was then ligated into the unique NcoI site that is present in the Idh open reading frame of plasmid, pLDH193. To minimize the possibility of re-circularization of the vector without an insert, the NcoI-digested pNEB193 was dephosphorylated with calf intestinal alkaline phosphatase prior to ligation. The ligation reaction mixture was introduced into Escherichia coli JM110 and the transformed cells were plated on LB medium that contained 20 μg/ml of tetracycline. Tetracycline-resistant tranformants that contained plasmids with the correct insert were identified by restriction digest analysis with NcoI, AsiSI, NotI, FseI, and PacI, and the orientation of the Tc^(r)-cassette was confirmed by PCR analysis using appropriate primers. A circle diagram of the plasmid that was selected for further manipulation (pLDHTc139#7) is shown in FIG. 12. In experiments not described here, this suicide construct was used to insertionally-inactivate (i.e. “disrupt” or “knockout”) the D-lactate dehydrogenase gene in ZW1 using host-mediated, double-crossover, homologous recombination and growth on tetracycline as the selection. Construction of pLDHTc139#7-9WW

Having demonstrated that pLDHTc139#7 could be used to “knockout” the D-lactate dehydrogenase gene in ZW1, the next step was to modify this construct so that it would be possible to remove the selectable marker from the chromosome after gene disruption, using Cre recombinase. To accomplish this goal, two wild type loxP sites (Lee and Saito, 1998) were added to pLDHTc139#7 taking advantage of the four unique restriction sites that flank the Tc^(r)-cassette, namely, AsiSI and NotI at the 5′ end and PacI and FseI at the 3′ end. The first loxP site was inserted between the AsiSI and NotI sites of plasmid pLDHTc139#7 after cutting the construct with both enzymes and purifying the resulting large DNA fragment. The loxP site that was inserted into this location was generated from two synthetic oligonucleotides 5 and 6 (SEQ ID NOs:21 and 22) that were both phosphorylated at their 5′ end.

Oligonucleotide 5 (SEQ ID NO:21); cgcATAACTTCGTATAATGTATGCTATACGAAGTTATgc Oligonucleotide 6 (SEQ ID NO:22); ggccgcATAACTTCGTATAGCATACATTATACGAAGTTATgcgat These oligonucleotides are complimentary to each other, and when annealed together form a full-length double-stranded wild type loxP site that has single-stranded overhangs at both ends, which allow the DNA fragment to be ligated between the AsiSI and NotI sites of pLDHTc139#7. The upper case letters in the oligonucleotides correspond to the full-length wild type loxP site, while the lower case letters indicate the nucleotides that were used to ligate the double-stranded DNA fragment into the AsiSI and NotI sites of pLDHTc139#7.

The ligation reaction mixture was used to transform E. coli DH10B and the transformed cells were plated on LB medium that contained 20 μg/ml of tetracycline. Tetracycline-resistant tranformants that contained plasmids with the loxP site correctly inserted into the AsiSI and NotI sites of pLDHTc139#7 were identified by restriction digest analysis, colony PCR, and DNA sequence analysis of the relevant regions. The plasmid that was selected for further manipulation is referred to below as pLDHTc139#7-9W.

Next, a second wild type loxP site was inserted between the PacI and FseI sites at the other end of the Tc^(r)-cassette in pLDHTc139#7-9W, after cutting the plasmid with both enzymes and purifying the resulting large vector fragment. The loxP site that was inserted into this location was also generated with two synthetic oligonucleotides 7 and 8 (SEQ ID NOs: 23 and 24) that were both phosphorylated at their 5′ end.

Oligonucleotide 7 (SEQ ID NO:23): taaATAACTTCGTATAATGTATGCTATACGAAGTTATggccgg Oligonucleotide 8 (SEQ ID NO:24): ccATAACTTCGTATAGCATACATTATACGAAGTTATttaat Oligonucleotides 7 and 8 are complimentary to each other, and when hybridized form a full-length, double-stranded wild type loxP site that has single-stranded overhangs at both ends that allow the DNA fragment to be ligated between the PacI and FseI sites of pLDHTc139#7-9W. The upper case letters in the oligonucleotides correspond to the full-length loxP site, and the lower case letters indicate the nucleotides that were used to ligate the double-stranded DNA fragment into the PacI and FseI sites of pLDHTc139#7-9W.

The ligation reaction mixture was used to transform E. coli DH10B and the transformed cells were plated on LB medium that contained 20 μg/ml of tetracycline. Tetracycline-resistant tranformants that contained plasmids with the wild type loxP site correctly inserted into the PacI and FseI sites of pLDHTc139#7-9W were identified by restriction digest analysis, colony PCR, and DNA sequence analysis of the relevant regions. The plasmid that was selected for further manipulation is referred to below as pLDHTc139#7-9WW, and a circle diagram of this construct is shown in FIG. 12.

Construction of pLDHSp-9WW

pLDHSp-9WW is identical to pLDHTc139#7-9WW, but the tetracycline-resistance cassette in the latter construct was replaced with a DNA fragment that confers resistance to spectinomycin (i.e. a Spec^(r)-cassette). The latter was generated by PCR using plasmid pHP15578 (Cahoon et al, 2003) as a template and Primers 9 and 10. pHP15578 contains the complete nucleotide sequence for the Spec^(r)-cassette and its promoter, which is based on the published sequence of the Tranposon Tn7 aadA gene (GenBank accession number X03403) that codes for 3′ (9)-O-nucleotidyltransferase.

Primer 9 ATAAAAgcggccgcAGCACAGGATGA (SEQ ID NO:25) Primer 10 GGCGttaattaaGGCAGGTCAGCAAG (SEQ ID NO:26)

The underlined bases of Primer 9 (forward primer) hybridize just upstream from the promotor for the Spec^(r)-cassette (to nts 6-17 of GenBank accession number X03043), while the lower case letters correspond to a NotI site that was added to the 5′ end of the primer. The underlined bases of Primer 10 (reverse primer) hybridize about 130 bases downstream from the stop codon for the Spec^(r)-cassette (to nts 1006-1019 of GenBank accession number X03043), while the lower case letters correspond to a PacI site that was added to the 5′ end of the primer. The 1040 bp PCR-generated Spec^(r)-cassette was double-digested with NotI and PacI, and the resulting DNA fragment was purified by agarose gel electrophoresis. Plasmid pLDHTc139#7-9WW was also cut with the same two

restriction enzymes to remove the Tc^(r)-cassette, and the resulting large vector fragment was purified by agarose gel electrophoresis. The two DNA fragments of interest were then ligated together, and the transformation reaction mixture was introduced into E. coli DH10B using electroporation. Transformants were plated on LB medium that contained spectinomycin (200 μg/ml) and grown at 37° C. Spectinomycin-resistant tranformants that contained plasmids with the correct size insert were identified by restriction digest analysis with NotI and PacI, and the plasmid that was selected for further manipulation is referred to below as pLDHSp-9WW; a circle diagram of this construct is shown in FIG. 12. In experiments not described here, pLDHSp-9WW was used to knockout the gene for D-lactate dehydrogenase in ZW1 using resistance to spectinomycin as the selectable marker. Gene inactivation with the suicide construct occurred via host-mediated, double-crossover, homologous recombination, (WO 01/83784 A2), which resulted in the insertion of the selectable marker (the Spec^(r)-cassette) that is flanked by two wild type loxP sites in the middle of the Idh open reading frame. The double-crossover event was targeted to the Idh gene by two DNA fragments that flank the Spec^(r)-cassette in pLDHSp-9WW. One of these fragments (referred to below as 5′ Idh flanking DNA) is just upstream from the Spec^(r)-cassette and is located between the SbfI and AsiSI sites. The nucleotide sequence of this ˜1100 bp DNA fragment is identical to the ZW1 chromosomal DNA that codes for the 3′ end of the pgm gene and about the first half of the Idh open reading frame. The other DNA fragment (referred to below as the 3′ Idh flanking DNA) is located at the opposite end the Spec^(r)-cassette between the FseI and AscI sites. The nucleotide sequence of the 3′ Idh flanking DNA (which is also ˜1100 bp) is identical to the chromosomal DNA that codes for the other half of the Idh gene and part of the 5′ non-translated region of the adhI gene. A double-crossover event occurs when the 5′ and 3′ Idh flanking DNA fragments both interact with their chromosomal counterparts and undergo homologous recombination. This phenomenon, which is essentially irreversible and entirely mediated by the host's enzymatic machinery, inactivates the chromosomal Idh gene by inserting the Spec^(r)-cassette in the middle of the open reading frame. Since the construct cannot replicate in Z. mobilis, making it a suicide construct, the only way to generate stable spectinomycin-resistant colonies with pLDHSp-9WW (apart from spontaneous drug resistant mutants that occur at a very low frequency) is a double-crossover event through homologous recombination. It is important to note that the Spec^(r)-cassette that gets inserted into the chromosome by the double-crossover event is still sandwiched between the two wild type loxP sites that were present in the suicide construct. Because of this arrangement it is easy to remove the selectable marker from the D-lactate dehydrogenase gene without reactivating it by using the Cre Expression vector that is described in Example 10. Construction of pGFORSp-9WW

pLDHSp-9WW was converted to a suicide construct for gene inactivation of Z. mobilis glucose-fructose oxidoreductase (GFOR) in a 2-step procedure as described below. The first step was to remove the 3′ Idh flanking DNA and replace it with an analogous DNA fragment that would target the plasmid construct to the chromosomal gene that codes for GFOR. The latter DNA fragment (referred to below as 3′ GFOR flanking DNA) was generated by PCR using ZW1 genomic DNA as a template and Primers 11 and 12 as PCR primers.

Primer 11 (SEQ ID NO:27) CTACTCATggccggccTCAGAACGATCCTGCACAGC Primer 12 (SEQ ID NO:28) CATCTTACTggcgcgccGGACGAGGTTCATCATCAGG The underlined bases of Primer 11 (forward primer) hybridize to nucleotides 684324-684305 of GenBank accession number AE008692 which are approximately in the middle of the GFOR open reading frame, while the lower case letters correspond to an FseI site that was added to the 5′ end of the primer. The underlined bases of Primer 12 (reverse primer) hybridize to nucleotides 683124-683143 of GenBank accession number AE008692 which is ˜625 bp downstream from the GFOR stop codon, while the lower case letters correspond to an AscI site that was added to the 5′ end of the primer. The 1234 bp PCR fragment was cut with FseI and AscI. pLDHSp-9WW was also cut with the same restriction enzymes to remove the 3′ Idh flanking DNA, and the large vector fragment resulting from this manipulation was purified by agarose gel electrophoresis. The PCR-generated 3′ GFOR flanking DNA was then ligated between the FseI and AscI sites of the gel purified large vector fragment described above, and an aliquot of the ligation reaction mixture was electroporated into E. coli DH10B. The transformed cells were plated on LB medium that contained 200 μg/ml of spectinomycin and the plates were incubated at 37° C. Spectinomycin-resistant transformants that contained plasmids with the correct insert were identified by colony PCR and restriction digestion analysis with FseI and AscI, and the plasmid that was selected for further manipulation is referred to below as pLDH/GFORSp-9WW.

The next step was to remove the 5′ Idh flanking DNA from pLDH/GFORSp-9WW and replace it with 5′ GFOR flanking DNA, so a double-crossover event could occur at the chromosomal targets that were selected for disruption of the GFOR open reading frame. The 5′ GFOR flanking DNA fragment was generated by PCR using ZW1 genomic DNA as a template and Primers 13 and 14 as PCR Primers.

Primer 13 (SEQ ID NO:29): CTACTCATatgcatGTCCAGAAAAGACAGCATTCC Primer 14 (SEQ ID NO:30): CATCTTACTgcgatcgcTGCACGGTTCATTGGAT The underlined bases of Primer 13 (forward primer) hybridize to nucleotides 685584-685564 of GenBank accession number AE008692 which are approximately 520 bp upstream from the GFOR start codon, while the lower case letters correspond to an NsiI site that was added to the 5′ end of the primer. The underlined bases of Primer 14 (reverse primer) hybridize to nucleotides 684396-684415 of GenBank accession number AE008692 which are close to the middle of the GFOR open reading frame and just upstream from the binding site for Primer 11, while the lower case letters correspond to an AsiSI site that was added to the 5′ end of the primer. The 1217 bp PCR product was cut with NsiI and AsiSI, and pLDH/GFORSp-9WW was double-digested with SbfI and AsiSI to remove the 5′ Idh flanking DNA; the large vector fragment resulting from the latter manipulation was purified by agarose gel electrophoresis. The PCR-generated 5′ GFOR flanking DNA was then ligated into the SbfI and AsiSI sites of the gel purified large vector fragment described above, and an aliquot of the ligation reaction mixture was electroporated into E. coli SCS110 (which is dcm⁻¹ and dam⁻) to obtain non-methylated plasmid DNA for subsequent transformation of ZW1 and ZW658, which is described in detail below in Examples 5 and 7. Note that the use of non-methylated plasmid DNA for transformation of Z. mobilis stains that are derived from ZM4 is critical for success, since methylated plasmid DNA that is isolated from wild type E. coli strains, like DH10B, is readily destroyed by the host's restriction/modification system (described in U.S. Pat. No. 6,566,107 B1). Note further that NsiI and SbfI have compatible sticky ends, but both sites are destroyed when they are ligated together. Transformants were plated on LB medium that contained 100 μg/ml of spectinomycin and the plates were incubated at 37° C. Spectinomycin-resistant transformants that contained plasmids with the correct insert were identified by colony PCR and restriction digestion analysis. This resulting suicide construct that was used to knockout the GFOR gene in ZW1 and ZW658 is referred to below as pGFORSp-9WW. A circle diagram of this plasmid is shown in FIG. 12, and its complete nucleotide sequence is disclosed in SEQ ID NO:31. It is important to note that a double-crossover event between this suicide construct and the Z. mobilis chromosome results in the insertion of a Spec^(r)-cassette that is flanked by two wild type loxP sites, analogous to the situation described above for pLDH-Spec-9WW.

Example 4 Generation of an E. coli Xylose Isomerase Expression Vector for Z. mobilis

A plasmid construct for expression of E. Coli xylose isomerase in Z. mobilis (pZB188/Kan-XylA) was generated as described below using an E. coli/Z. mobilis shuttle vector (pZB188) as starting material (FIG. 13). Steps involved in the construction of pZB188 are disclosed in U.S. Pat. No. 5,514,583. Briefly, this 7008 bp plasmid is able to replicate in E. coli and Z. mobilis because it has two different origins of replication, one for each bacterial species. pZB188 also contains a DNA fragment that confers resistance to tetracycline (i.e. a Tc^(r)-cassette). The first step in the construction of pZB188/Kan-XylA, was to remove the Tc^(r)-cassette from pZB188 and replace it with a DNA fragment that confers resistance to kanamycin (i.e. Kan^(r) cassette). To excise the Tc^(r)-cassette from pZB188, the plasmid was cut with XbaI and BssHII and the resulting large vector fragment was purified by agarose gel electrophoresis. The Kan^(r)-cassette was generated by PCR using plasmid pET-24a (Novagen) as a template and Primers 15 and 16 for PCR-amplification. pET-24a contains the complete open reading frame for the Kan^(r) gene and its associated promoter.

Primer 15 (SEQ ID NO:32): GCtctagaGCAGCAGATTACGCGC Primer 16 (SEQ ID NO:33): ACATTGgcgcgcTTAGAAAAACTCATC The underlined bases of Primer 15 (forward primer) hybridize about 160 bp upstream from the start codon for the Kan^(r) gene in pET-24a, while the lower case letters correspond to an XbaI site that was added to the 5′ end of the primer. The underlined bases of Primer 16 (reverse primer) hybridize at the other end of the open reading frame for the Kan^(r) gene and include the termination codon, while the lower case letters correspond to a BssHII site that was added to the 5′ end of the primer. The 991 bp PCR-generated Kan^(r)-cassette was cut with XbaI and BsshII, and purified by agarose gel electrophoresis.

The resulting DNA fragment was then inserted between the XbaI and BssHII sites of the pZB188 DNA fragment described above in a standard ligation reaction. The transformation reaction mixture was introduced into E. coli DH10B using electroporation and the cells were plated on LB medium that contained kanamycin (50 μg/ml); growth was at 37° C. Plasmid DNA was isolated from one of the kanamycin-resistant transformants, and the resulting construct is referred to below as pZB188/Kan; a circle diagram of this shuttle vector is shown in FIG. 13.

In the next step, an E. coli xylose isomerase expression cassette was inserted between the NcoI and AcII sites of pZB188/Kan after cutting the latter with both enzymes, and purifying the large vector fragment by agarose gel electrophoresis. The ˜2 Kbp DNA fragment that served as the E. coli xylose isomerase expression cassette was derived from plasmid pZB4 after cutting the latter construct with NcoI and ClaI, and purifying the relevant DNA fragment by agarose gel electrophoresis. Plasmid pZB4 is described in detail in U.S. Pat. No. 5,514,583, and a schematic representation of the E. coli expression cassette P_(gap)XylA (SEQ ID NO:34) is shown in the boxed diagram of FIG. 13.

NcoI and ClaI sites were located at the 5′ and 3′ ends, respectively, of the E. coli xylose isomerase expression cassette. As described in U.S. Pat. No. 5,514,583, this fragment contains the strong, constitutive Z. mobilis glyceraldehyde 3-phosphate dehydrogenase (GAP) promoter, which is precisely fused to the complete open reading frame of the E. coli xylA gene that codes for xylose isomerase. It also contains the small stem-loop region that immediately follows the xylose isomerase stop codon. The E. coli xylose isomerase expression cassette was inserted between the NcoI and AclI sites of pZB188/Kan in a standard ligation reaction. Note that ClaI and AclI generate compatible “sticky ends”, but both sites are destroyed when they are ligated together. The ligation reaction mixture was then electroporated into E. coli SSC110 (dcm⁻¹, dam⁻) to obtain non-methylated plasmid DNA for subsequent transformation of Z. mobilis as described below in Example 6, and transformed cells were plated on LB medium that contained kanamycin (50 μg/ml); growth was at 37° C. Kanamycin-resistant tranformants that had a plasmid with a correct size insert were identified by restriction digestion analysis and colony PCR. The plasmid that was used to express E. coli xylose isomerase in Z. mobilis is referred to below as “pZB188/Kan-XylA”; a circle diagram of this construct is shown in FIG. 13.

Example 5 Generation of the ZW1 GFOR Knockout Mutant

To eliminate GFOR enzyme activity in ZW1 (the wild type strain that ZW658 was originally derived from) the suicide construct pGFORSp-9WW, which was described in detail in Example 3, was used. The non-replicating plasmid DNA was introduced into the bacterial host using electroporation, essentially as described in U.S. Pat. No. 5,514,583. Briefly, the 50-μl transformation reactions contained ˜10¹⁰ cells/ml in 10% (v/v) glycerol and ˜0.9 μg of non-methylated plasmid DNA that was isolated from E. coli SSC110 as described in Example 3. The control reaction was treated identically, but did not receive any plasmid DNA. The settings for the electroporator were 16 kv/cm, 200Ω, and 25 μF, and the gap width of the cuvette was 0.1 cm. After electroporation, the transformation reactions were diluted with 1.0 ml of MMG media (50 g/L glucose, 10 g/L yeast extract, 5 g/L of tryptone, 2.5 g/L of (NH₄)₂SO₄, 0.2 g/L K₂HPO₄, and 1 mM MgSO₄) and the cells were allowed to recover for ˜5 hours at 30° C. The cells were then harvested by centrifugation at room temperature (13,000×g, 5 min) in sterile 1.5-ml microfuge tubes and the supernatants were carefully removed. Cell pellets were resuspended in 150 μl of liquid MMG media, and 50- and 100-μl aliquots of the cell suspension were plated on MMG medium that contained 1.5% agar and 200 μg/ml of spectinomycin. The plates were incubated in an anaerobic chamber at 30° C., and 50 to 150 colonies appeared on the experimental plates after 2 to 3 days. No spectinomycin-resistant colonies were on the control plates at this time, although a few appeared after another 48-hr incubation period. Two of the spectinomycin-resistant colonies that resulted from transformation with the GFOR knockout construct were selected for further manipulation as described below.

Previous experiments with Z. mobilis and suicide constructs that are similar to pGFORSp-9WW have revealed that the initial interaction between the chromosome and the plasmid DNA is a single-crossover event at one of the two targeted loci, and that single-crossover events eventually give rise to double-crossover events. Transition to the double-crossover event normally occurs very rapidly after a few serial transfers in liquid medium that contains the selective agent for the suicide construct. To facilitate the double-crossover event for the two selected ZW1 transformants that resulted from the GFOR knockout construct, cells were inoculated into 10 ml of RM media (10 g/L of yeast extract and 2 g/L of KH₂PO₄) that contained 100 g/L of glucose and 200 μg/ml of spectinomycin. Both cultures reached stationary phase after a 24-hr incubation period at 30° C. Next, 10 μl-aliquots of the 1^(st)-pass cultures were used to inoculate 10 ml of the same growth medium, and both of these cultures also reached stationary phase after 24 hrs at 30° C. Finally, 10-μl aliquots of the 2^(nd)-pass cultures were inoculated into 10 ml of the same growth medium and growth was allowed to proceed for another 24 hrs at 30° C. Following the last transfer in liquid medium, aliquots of the 3^(rd)-pass cultures were diluted and plated on MMG medium that contained spectinomycin (200 μg/ml) to obtain single colonies, and the plates were incubated at 30° C. for 48 hr under anaerobic conditions.

Confirmation that the double-crossover event had indeed occurred was obtained from colony PCR experiments using three different pairs of primers. The first pair of PCR primers can only generate a DNA fragment of the correct size if the 5′ GFOR flanking DNA in the suicide construct has undergone a single-crossover event with its chromosomal counterpart. Similarly, the second pair of PCR primers can only generate a DNA fragment of the correct size if the 3′ GFOR flanking DNA in the suicide construct has undergone a single-crossover event with its chromosomal counterpart. Finally, the third pair of PCR primers can only generate a DNA fragment of the correct size if a double-crossover event has occurred and in addition rules out the possibility of a mixed population of single- and double-crossover events. The two spectinomycin-resistant colonies that were used for this analysis were derived from two different primary transformants from the ZW1 electroporation reaction with the suicide construct that were transferred three times in liquid medium and plated to obtain single colonies as described above, and the control for this experiment was the parent strain, ZW1. Since both transformants yielded positive results with the three different sets of PCR primers, only one of them was selected for further analysis. This strain (the ZW1 GFOR knockout mutant) is referred to below as ZW1-ΔGFOR.

Example 6 Glucose-Fructose Oxidoreductase can be a Major Contributor to Xylitol Formation Under Physiological Conditions

The ZW1 GFOR knockout mutant (ZW1-ΔGFOR) was used to test the hypothesis that xylitol formation in xylose-utilizing, recombinant strains of Z. mobilis is at least partially mediated by the periplasmic enzyme GFOR, or its larger molecular weight cytosolic precursor which is also enzymatically active (Loos et al., supra). As shown in Example 2 (FIG. 11), xylitol is a major by-product of xylose-utilizing strains 8b and ZW658, but is only formed when xylose is present in the growth medium. Although wild type strains of Z. mobilis, like CP4, have an NADPH-dependent aldose reductase that can directly reduce xylose to xylitol (Feldmann et al, supra), it is conceivable that GFOR could also contribute to xylitol formation in vivo when the growth medium contains xylose or a mixture of glucose and xylose as depicted in Diagrams II and III. However, for either of these reactions to occur the enzyme would need access to xylulose, since this compound is the obligatory electron acceptor for GFOR-mediated xylitol production as shown in in vitro GFOR enzyme characterization assays (Zachariou and Scopes, supra). In Z. mobilis strains that are engineered for growth on xylose, the xylulose that would be necessary for xylitol synthesis would be generated by xylose isomerase, which catalyzes the first step of xylose metabolism (FIG. 1) and is absent in wild type strains, like ZW1

To test the possibility that GFOR can generate xylitol when xylose and glucose are both present in the growth medium, the E. coli xylose isomerase expression vector (pZB188/Kan-XylA) that was described in Example 4 was introduced into ZW1 and ZW1-ΔGFOR. The strategy was to provide a route from xylose to xylulose in two strains that cannot grow on either of these sugars and determine whether GFOR could generate xylitol. The electroporation procedure that was used for transformation was essentially as described in Example 5, but after the recovery period the transformed cells were plated on MMG medium that contained 300 μg/ml of kanamycin. As controls for this experiment, ZW1 and ZW1-ΔGFOR were also transformed with pZB188/Kan (FIG. 13), which is identical to pZB188/Kan-XylA but lacks the E. coli xylose isomerase expression cassette. Kanamycin-resistant colonies harboring the pZB188/Kan-XylA or the control plasmid were identified by colony PCR, and a representative colony from each transformation reaction was randomly selected for the experiment that is shown in FIG. 14. These four plasmid-bearing strains are referred to below as ZW1 (pZB188/Kan), ZW1 (pZB188/Kan-XylA), ZW1-ΔGFOR(pZB188/Kan) and ZW1-ΔGFOR (pZB188/Kan-XylA).

Overnight cultures were grown in 15-ml capped test tubes at 30° C. in 5 ml of 60 g/L glucose, 10 g/L yeast extract, 10 g/L KH₂PO₄, 2 g/L (NH₄)₂SO₄, 1 g/L MgSO₂(7H₂O) and 300 μg/ml of kanamycin. Aliquots of these overnight cultures were then used to inoculate 20 ml cultures (in 50-ml capped test tubes) that contained the same growth medium, with or without 20 g/L of xylose. Growth was at 30° C. with gentle agitation, and initial OD₆₀₀ values were ˜0.1. After 0, 24, 48, and 120 hours of growth, 1.0-ml aliquots of the cultures were removed for HPLC analysis using an HP 1100 equipped with a refractive index detector (Hewlett-Packard, Palo Alto, Calif.) to determine the concentrations of xylose, xylulose and xylitol that were present in the fermentation broth. Prior to HPLC analysis, cells were removed by centrifugation and the supernatant was filtered through a 0.22 μm cellulose acetate Spin-X centrifuge tube filter (Costar, catalog number 8160) to remove small particles. Compounds were separated on an Aminex HPX-87H column (Bio-Rad) that was run at 55° C. under isocratic conditions using a flow rate of 0.6 ml/min and 0.01 NH₂SO₄ as the mobile phase. Authentic standards of known concentration were used to quantify the peaks of interest and all results are expressed in g/L.

The results show that when ZW1 (pZB188/Kan), the control strain with the “empty” vector, was grown in the presence of glucose and xylose, only a small amount of xylitol accumulated in the growth medium after a 120-hr incubation period (FIG. 14A). The maximum amount of xylitol that was observed with this strain was <0.5 g/L. In contrast, no xylitol was formed when ZW1 (pZB188/Kan) was grown in the same concentration of glucose but xylose was omitted, and this was true for the other three strains as well. Consequently, only the experiments that were performed in the presence of both glucose and xylose are shown in FIG. 14. Remarkably, expression of E. coli xylose isomerase in ZW1 greatly increased the amount of xylitol that appeared in the fermentation broth, and by 120 hours ZW1 (pZB188/Kan-XylA) had generated five times more of this compound than ZW1(pZB188/Kan) (FIG. 14B). As anticipated, expression of xylose isomerase in ZW1 also resulted in the production of xylulose, since xylose isomerase catalyzes the isomerization of xylose to xylulose. Note that in this experiment approximately 16% of the total xylose that was added to the growth medium was converted to xylulose or xylitol. Also note that there is an apparent precursor/product relationship between these two compounds (xylulose decreased as xylitol increased), consistent with the hypothesis that GFOR is able to convert xylulose to xylitol under physiological conditions when glucose and xylose are both present in the growth medium.

Similar to ZW1, very little xylitol was generated by ZW1-ΔGFOR in the absence of the xylose isomerase expression vector (FIG. 14C). The small amount of xylitol that was formed under these conditions may come from an NADPH-dependent aldose reductase, as suggested by Feldmann et al. (1992 supra). Strikingly, when xylose isomerase was expressed in the ZW1 GFOR knockout mutant, no additional xylitol was generated (FIG. 14D), in contrast to the results that were obtained with ZW1 (pZB188/Kan-XylA). Instead, ZW1-ΔGFOR (pZB188/Kan-XylA) produced massive amounts of xylulose, and the amount of this compound that was formed was very similar to the total amount of xylulose and xylitol that was generated by the corresponding ZW1 stain (i.e. ZW1(pZB188/Kan-XylA)). These experiments clearly demonstrate that GFOR can substantially contribute to xylitol formation in vivo when the enzyme has access to xylulose, which is certainly the case for xylose-utilizing, recombinant strains of Z. mobilis that are grown in mixtures of glucose and xylose. These results further indicate that NADPH-dependent aldose reductases play a minor role in xylitol production when recombinant strains of Z. mobilis are grown in xylose-containing media, contrary to expectations from the literature (Feldmann et al, supra; Kim et al, supra).

Example 7 Generation of the ZW658 GFOR Knockout Mutant and Demonstration that this Strain does not Produce a Functional GFOR Enzyme

The gene encoding GFOR, which can contribute to xylitol formation in Z. mobilis under physiological conditions when glucose and xylulose are both available as shown in Example 6, was insertionally-inactivated in ZW658 using the suicide construct, pGFORSp-9WW (described in Example 3). All steps in this procedure were identical to those described for the ZW1 GFOR knockout mutant in Example 5, including confirmation of the double-crossover event with the three sets of PCR primers. The ZW658 knockout mutant that was chosen for subsequent experiment described below was named ZW800.

To demonstrate that ZW800 does not produce an enzyme that can generate sorbitol from glucose and fructose, which is the physiological reaction that is catalyzed by GFOR, the following experiment was performed. One and a half milliliter cultures of ZW800 and the parent strain ZW658 were grown to early stationary phase in 10-ml capped test tubes at 30° C. in liquid medium that contained 75 g/L glucose, 25 g/L xylose, 10 g/L yeast extract, 2 g/L of KH₂PO₄, and 1 g/L MgSO₄. When the cultures reached an OD₆₀₀ of ˜5.5, cells were harvested by centrifugation and the supernatant was carefully removed and discarded. Next, the cell pellets were resuspended in 5 ml of fresh growth medium that had the following composition: 110 g/L glucose, 110 g/L fructose, 10 g/L yeast extract, 2 g/L of KH₂PO₄, 1 g/L MgSO₄, and 4 g/L KHCO₃. All steps above were performed under sterile conditions and the initial pH of the growth medium was adjusted to 5.8 with concentrated phosphoric acid before the cells were resuspended. The resulting cultures were then grown at 30° C. with gentle agitation (150 rpm) and at times indicated in Table 2, samples were removed for HPLC analysis of the fermentation broth using the same procedure that was described in Example 6. The peaks of interest for this experiment were glucose, fructose, sorbitol and ethanol, and authentic standards of known amount were used to calculate their concentrations in the fermentation broth after cells were removed by centrifugation; all concentrations are expressed in g/L in Table 2.

TABLE 2 Sorbitol production in ZW658 and ZW800 - in vivo measurements. Strain Hour Glucose Fructose Sorbitol Ethanol ZW658 0 110 110 0 0 ZW658 23 5.99 61.43 45.99 49.36 ZW658 47 1.55 21.98 45.89 69.04 ZW800 0 110 110 0 0 ZW800 23 0 60.44 0 73.85 ZW800 47 0 6.79 10.21 96.21

As shown in Table 2, the ZW658 culture consumed almost all of the glucose and about half of the fructose after 23 hr and generated comparable amounts of sorbitol and ethanol as major products; the values for the two latter compounds during the first time point were 45.99 g/L and 49.36 g/L, respectively. Thus, more than 40% of the original fructose was converted to sorbitol by GFOR in the ZW658 culture. In striking contrast, no sorbitol was detected in the fermentation broth from the ZW800 culture after a 23-hr incubation period, and instead the glucose and fructose were almost quantitatively converted to ethanol, which was very close to the theoretical value of 0.51 grams of ethanol per gram of sugar consumed. Note that there was no further increase in the amount of sorbitol in the ZW658 culture after another 24 hours of growth. This was expected since nearly all of the glucose was depleted earlier and there was no electron donor for the GFOR reaction with fructose. Interestingly, a small amount of sorbitol (10.21 g/L) was found in the fermentation broth of the ZW800 culture at the 47-hr time point, and this may have been generated by an NADPH-dependent aldose reductase (Feldmann et al., supra) or some other enzyme that remains to be elucidated. Nevertheless, the above results provide evidence that the Spec^(r)-cassette that was inserted in the middle of the GFOR open reading frame of ZW800 largely, if not entirely, abolished GFOR enzyme activity.

Further support for this conclusion comes from in vitro experiments with cell-free extracts that were prepared from ZW1, ZW658 and ZW800. The goal was to determine if ZW658 can convert xylose to xylitol in the absence of other added substrates or co-factors, and to see if ZW800 has lost the ability to carry out this reaction as a result of GFOR inactivation. There are three requirements for GFOR-mediated xylitol production with Z. mobilis cell-free extracts: 1) a sugar electron donor like glucose or xylose that is able to reduce the GFOR's tightly bound co-factor, 2) xylulose as an electron-acceptor, since it is the compound that the enzyme actually reduces to xylitol, and 3) a functional GFOR enzyme. If xylulose is not added to the reaction mixture, the cell-free extract must also contain xylose isomerase to convert xylose to xylulose.

Cell-free extracts were prepared from 100-ml cultures that were grown at 33° C. in 250-ml shake flasks that contained 10 g/L yeast extract, 2 g/L KH₂PO₄ and 50 g/L glucose. Cells were harvested by centrifugation at an OD₆₀₀ between 2-3 and were washed twice with ice-cold 50 mM Tris-HCl (pH 7.0), 1.0 mM MgCl₂, 1 mM dithiothreitol. The final pellets were resuspended in 1.0 ml of the same buffer and cells were disrupted by sonication. After cell debris was removed by centrifugation at 4° C. (16,000×g, 60 min), the cell-free extracts were immediately assayed for xylitol production as described below. The 500-μl reactions were conducted in polypropylene microfuge tubes and contained final concentrations of the following components: 50 mM Tris-HCl (pH 7.0), 1.0 mM MgCl₂, 1 mM dithiothreitol, 66 mM xylose, and 0.32-0.35 mg of cell-free extract protein; protein concentrations were determined by the BCA Protein Assay (Pierce) using bovine serum albumen as a standard. Following a 15-hr incubation period at 40° C., reactions were terminated with a final concentration of 30 mM pivalic acid and aliquots were analyzed by HPLC using a SH1011 column (Showdex) with 0.01N sulfuric acid as the mobile phase. The column temperature was maintained at 50° C. and the flow rate was 1.0 ml/min. The control for this experiment did not receive cell-free extract, but was otherwise treated identically.

As shown in Table 3, when the ZW1 cell-free extract was added to the reaction mixture, xylose was not converted to xylulose or xylitol during the 15-hr incubation period. As already noted, this result was expected since ZW1 is a wild type strain that does not express E. coli xylose isomerase, in contrast to ZW658 and ZW800. In contrast, significant amounts of xylulose and xylitol were generated when the ZW658 cell-free extract was used, since it contained both enzymes that are necessary for the formation of these two compounds. Note that in this case nearly 8% of the original 66 mM xylose was used for xylitol production, since two molecules of xylose are consumed for each molecule of xylitol that is generated when xylose is the only GFOR substrate that is added to the reaction mixture. Finally, and most important, the ZW800 cell-free extract was only able to convert xylose to xylulose, since although it contained xylose isomerase activity, it lacked GFOR enzyme activity. These results provide additional evidence that ZW800 does not produce a functional GFOR enzyme and further demonstrate that this protein is able to use xylose as an electron donor to reduce xylulose to xylitol, as previously shown with wild type cell-free extracts that were spiked with purified xylose isomerase (Danielson supra).

TABLE 3 GFOR-mediated production of xylitol from xylose also requires xylulose - in vitro measurements Cell-free extract Xylulose (mM) Xylitol (mM) none 0 0 ZW1 0 0 ZW658 9.45 2.6 ZW800 10.63 0

Example 8 Sorbitol is Needed for Growth of ZW800 in Concentrated Mixtures of Glucose and Xylose

The fermentation performance for production of ethanol by ZW800 in a concentrated mixture of glucose and xylose was tested. The experiments were conducted in pH-controlled fermentors using a fixed glucose to xylose ratio of ˜5:4 at 97 g/L or 188 g/L of total sugar.

Seed cultures of ZW658 and ZW800 were grown in shake flasks at 37° C. in liquid medium that contained 75 g/L glucose, 25 g/L xylose, 10 g/L yeast extract, 10 g/L KH₂PO₄, 2 g/L (NH₄)₂SO₄, and 1 g/L MgSO₄; initial pH was adjusted to 5.5 with 4 N KOH. When the OD₆₀₀ reached ˜5.0, 50-ml aliquots of the seed cultures were used to inoculate 1-liter fermentors (BIOSTAT® B-DCU system, Sartorius BBI System Inc., Bethlehem, Pa., USA) that contained 450 ml of growth medium. The final 500-ml cultures contained 5 g/L yeast extract, 2 g/L KH₂PO₄, 2 g/L (NH₄)₂SO₄,1 g/L MgSO₄ and either a low concentration of sugar (54 g/L glucose, 43 g/L xylose) or a high concentration of sugar (104 g/L glucose, 84 g/L xylose). Growth was at 33° C. and pH was maintained at 5.5 by automated addition of 4 N KOH. The mixing speed was set at 150 rpm. At various times, aliquots were removed for HPLC analysis of the fermentation broth using the same procedure and conditions that were described in Example 6. The compounds of interest for this experiment were glucose, xylose, and ethanol, and authentic standards of known concentration were used to quantify peaks on the chromatograms. Cell growth was also monitored by following changes in turbidity with a spectrophotometer that was set at an optical density of 600 nm, and the resulting OD₆₀₀ values were plotted.

As shown in FIG. 15, GFOR inactivation had no effect on growth, sugar consumption, or ethanol titer when the fermentor contained a low concentration of sugar (54 g/L glucose, 43 g/L xylose). However, a big difference in fermentation performance was observed when the total sugar concentration was increased about 2-fold as seen in FIG. 16. ZW658 experienced a lag period of about 30 hours, which is typical for xylose-utilizing recombinant strains of Z. mobilis when they are shifted from a dilute mixture of glucose and xylose to a concentrated mixture of the same sugars that exceeds ˜180 g/L of total sugar. Following the lag period, the cells started to grow and consumed all of the glucose in the medium and about 75% of the xylose, thus resulting in a final ethanol titer of ˜73 g/L (FIG. 16A). In contrast, the ZW800 culture did not recover from the lag period even after a 130-hr incubation period (FIG. 16B), and this result was obtained on two separate occasions.

Since ZW800 grew well in the dilute mixture of glucose and xylose as shown in FIG. 15, it seemed possible that the inability of this strain to recover in the high sugar mixture was somehow related to osmotic stress. Indeed, GFOR plays a critical role in maintaining osmotic balance by generating sorbitol when wild type Z. mobilis is transferred to concentrated mixtures of glucose and fructose or high concentrations of sucrose, which also gives rise to glucose and fructose through the action of invertase (Loos et al., supra). The sorbitol that is produced by GFOR in the periplasmic space is transported into cells against a concentration gradient where it accumulates to high levels since it is not further metabolized. This eliminates the osmotic pressure difference across the plasma membrane and restores osmotic balance (Wiegert et al., supra). However, a prerequisite for GFOR-mediated sorbitol production is the simultaneous presence of glucose and fructose, and this reaction should not occur in growth media that lacks fructose. Nevertheless, since sorbitol is the physiologically important product of GFOR and this enzyme is inactive in ZW800, the effect of adding sorbitol to the concentrated mixture of glucose and xylose was tested in the experiment described below.

After ˜70 hours in the high sugar mixture (time point designated by vertical arrow in FIG. 16), five 4.5-ml aliquots of the stalled ZW800 culture were removed from the fermentor and transferred to 15-ml capped test tubes. Four of the tubes were then supplemented with 0-20 mM sorbitol (final concentration), and the total volume of the cultures was adjusted to 5.0 ml with deionized water in all cases; the sorbitol stock solution that was used for this experiment was also made up in water. To control for the 10% dilution of the growth medium when the water and sorbitol were added, nothing was added to the fifth culture. All of the cultures were then incubated at 33° C. with gentle agitation (200 rpm) and growth was monitored spectrophotometrically. The cells started to grow almost immediately when sorbitol was added to the growth medium as shown in FIG. 17, even with the lowest concentration tested (5 mM). Some stimulation of growth was also observed when sorbitol was not added but the culture was diluted 10% with water, which reduced the total sugar concentration from 188 g/L to 169 g/L. However, the stimulatory effect of sorbitol on growth was much greater than the effect of dilution.

The rescue of ZW800 growth by sorbitol was completely unexpected since ZW658 recovered from the lag period and grew well in the concentrated mixture of glucose and xylose, without a known source of fructose. Since the latter compound is an obligatory electron acceptor for GFOR-mediated sorbitol production, it was not apparent that GFOR could synthesize sorbitol or play a role in osmotic balance in media that contain high concentrations of glucose and xylose. Thus there was no indication that sorbitol might be an important factor for growth of ZW658 or ZW800 in concentrated mixtures of glucose and xylose.

Example 9 GFOR Inactivation Improves Ethanol Production from Xylose Under Process Relevant Conditions

Fermentation performances of ZW658 and ZW800 in concentrated mixtures of glucose and xylose under process relevant conditions were compared in a side-by-side manner to determine whether GFOR inactivation is a beneficial or detrimental metabolic engineering strategy. Since high concentrations of glucose and xylose were used in these experiments, sorbitol was added to the medium to allow growth of ZW800. In experiments that are not described here, it was also discovered that sorbitol eliminates the lag period for ZW658. Thus, sorbitol supplementation of the growth medium provides an ideal way to compare these two strains under process relevant conditions.

ZW658 and ZW800 were compared under six different conditions using two concentrations of total sugars, in the presence and absence of acetate, and for the more concentrated sugar mixture, two different buffering capacities were examined. These experiments were conducted with 20-ml cultures that were grown at 30° C. in 50-ml test tubes with gentle agitation (150 rpm). pH was not controlled, but the initial pH of the growth medium was adjusted to 5.8 with concentrated phosphoric acid prior to inoculation with the seed culture. The basic growth medium contained 10 g/L yeast extract, 2 g/L KH₂PO₄, 1 g/L MgSO₄, 5 mM sorbitol and either 4 g/L (FIGS. 18 and 19) or 8 g/L (FIG. 20) of KHCO₃. All values given above and below are final concentrations after the seed culture was added. The KHCO₃ was used to increase the buffering capacity of the growth medium to minimize the drop in pH that normally occurs during bacterial growth. The carbon source for all of these experiments was a mixture of glucose and xylose that approximated the ratio of these two sugars in pre-treated corn stover hydrolysate at two different concentrations of total sugar. Initial concentrations of glucose and xylose were either 92 g/L and 82 g/L, respectively (FIG. 18) or 107 g/L and 96 g/L (FIGS. 19 and 20). Where indicated, 6 g/L of acetate (an inhibitor that is present in pre-treated corn stover hydrolysate) was also present. The seed culture was grown at 30° C. to an OD₆₀₀ of ˜5.0 in liquid media that contained 75 g/L glucose, 25 g/L xylose, 10 g/L yeast extract, 2 g/L KH₂PO₄, 1 g/L MgSO₄, and 1/10^(th) volume was used to inoculate the experimental cultures. At various times, aliquots were removed for HPLC analysis of the fermentation broth as previously described in Example 6. The compounds of interest for this experiment were glucose, xylose, ethanol and xylitol, and all values are reported in g/L. Since virtually all of the glucose was consumed before the first time points were taken, the values for this sugar were not plotted in the graphs.

From the experiments that are shown in FIGS. 18-20, it is clear that ZW800 outperformed ZW658 under all conditions tested as judged by two different criteria: (a) the total amount of xylose that was consumed during the course of the experiment, and (b) the maximum ethanol titer that was achieved. It is also evident from this data that the beneficial effects of GFOR inactivation largely occurred during the late stage of fermentation when the most stressful conditions were encountered (i.e. after all of the glucose was depleted and the ethanol concentration started approaching toxic levels). Indeed, the most striking differences between the two strains were observed when an inhibitory concentration of acetate was present in the growth medium, which constitutes an additional stress. The average increase in ethanol titer for ZW800 in the presence of acetate for the three sets of experimental conditions was 10.2% with values ranging from 4.4% to 13.7%. ZW800 also produced more ethanol than ZW658 in the absence of acetate in all three experiments, with the average increase in this case being 3.2%. As anticipated, ZW658 converted significant amounts of xylose to the unwanted by-product xylitol, and the highest levels of this compound were observed when conditions were the most stressful (i.e. during the late stages of fermentation and when acetate was present in the growth medium). For example, in the experiments with acetate that are shown in FIGS. 18-20, ZW658 converted 8.1%, 8.3% and 9.9% of the total xylose that was consumed to xylitol. In contrast, no xylitol was found in the ZW800 cultures under any of the conditions that were tested. These results clearly show that GFOR inactivation is beneficial to xylose metabolism for ethanol production under process relevant conditions, especially in the presence of inhibitory concentrations of acetate. The test tube experiments that are shown in FIGS. 18 and 19 were performed twice and virtually identical results were obtained.

Another side-by-side experiment with ZW800 and ZW658 in a concentrated mixture of glucose and xylose with acetate was performed using pH-controlled fermentors. By-products of metabolism such as organic acids and carbon dioxide produced by Z. mobilis can lower the pH, of the growth medium which increases the ratio of acetic acid to acetate, and it is known that the protonated species is the compound that actually inhibits bacterial growth (Kim et al, (2000) Applied Biochemistry and Biotechnology, 84-86:357-370). Thus, pH control is very important in large-scale fermentation, since a drop in pH from 5.8 to 5.0 would result in about a 5-fold increase in the concentration of acetic acid.

Seed cultures for ZW800 and ZW658 were grown in shake flasks at 37° C. in liquid medium that contained 75 g/L glucose, 25 g/L xylose, 10 g/L yeast extract, 10 g/L KH₂PO₄, 2 g/L (NH₄)₂SO₄, and 1 g/L MgSO₄; initial pH was adjusted to 5.5 with 4 N KOH. When the OD₆₀₀ reached ˜5.0, 50-ml aliquots of the seed cultures were used to inoculate 1-liter fermentors (BIOSTAT® B-DCU system, Sartorius BBI System Inc., Bethlehem, Pa., USA) that contained 450 ml of growth medium. The final 500-ml cultures contained 92 g/L glucose, 97 g/L xylose, 10 g/L yeast extract, 2 g/L KH₂PO₄, 10 mM sorbitol and 7.2 g/L of acetate. Growth was at 33° C. and pH was maintained at 5.5 by automated addition of 4 N KOH; the mixing speed was 150 rpm. At various times, aliquots were removed for HPLC analysis of the fermentation broth using the same procedure that is described in Example 6. The compounds of interest for this experiment were glucose, xylose, ethanol and xylitol, and cell growth (OD₆₀₀) was also monitored. FIG. 21 shows the full time course for these parameters for the fermentor run with the ZW800 culture and Table 4 summarizes end-point values for xylose, ethanol and xylitol for both strains.

TABLE 4 End-point values for xylose, ethanol, and xylitol in pH-controlled fermentors with ZW800 and ZW658. ZW658 ZW800 Ethanol (g/L) 65.95 72.31 Xylose consumed (g/L) 60.71 69.14 Xylitol (g/L) 3.92 0 Ethanol yield (g ethanol/g sugar) 0.43 0.45

Similar to the test tube results with acetate (FIGS. 18-20), ZW800 consumed 14% more xylose and generated 9.6% more ethanol than ZW658 in the pH-controlled fermentors (FIG. 21). The ethanol yield for ZW800 was also ˜5% higher since this strain did not produce any detectable xylitol. In contrast, the final concentration of xylitol in fermentation broth for ZW658 was 3.92 g/L, which represents ˜6.5% of the total xylose that was consumed during the course of the experiment. These experiments provide additional evidence that GFOR inactivation improves ethanol production from xylose by eliminating xylitol formation. As already noted, the unwanted by-product xylitol interferes with xylose metabolism in at least two different ways and inhibits bacterial growth, which results in lower levels of ATP. Thus, when GFOR generates xylitol it reduces the ability of Z. mobilis to cope with all of the other energy-consuming stresses that it normally encounters during ethanol production from lignocellulose feedstocks. Since ZW800 does not have to contend with xylitol-related stresses in contrast to ZW658, it consumes more xylose, produces more ATP and generates more ethanol during the late stage of fermentation when the highest level of stress is encountered.

Example 10 Removing the Selectable Marker from ZW800 and Characterization of the Resulting Strain, ZW801-4

Generation of the Cre-Expression Construct, pZB188-Kan/Cre

As described in Example 3, the Spec^(r)-cassette that was inserted into the GFOR open reading frame in ZW800 is sandwiched between two wild type loxP sites. This arrangement makes it easy to remove the selectable marker from the chromosome by using Cre Recombinase (Sternberg and Hamilton (1981) J. Mol. Biol. 150:467-486; Lee and Saito, supra; Trinh et al. (2000) Journal of Immunological Methods 244(2):185-193). In order to do this, however, it was first necessary to generate a Cre Expression vector that can replicate in Z. mobilis (FIG. 22). The precursor for the Cre Expression vector was pZB188/Kan, which was described in detail in Example 4. Briefly, pZB188/Kan is a shuttle vector that can replicate in E. coli and Z. mobilis because it has an origin of replication for both bacterial species. It also contains a DNA fragment that confers resistance to kanamycin (i.e. a Kan^(r)-cassette). pZB188/Kan was double-digested with NcoI and NotI, and the large vector fragment was purified by agarose gel electrophoresis. The next step was to generate a Cre-expression cassette and this was accomplished by PCR using primers 17 and 18. The DNA template that was used for amplification of the Cre-expression cassette was a plasmid that contained the full-length gene for the bacteriophage PI Cre Recombinase including its promoter (Sternberg et al. (1986) J. Mol. Biol. 187(2):197-212)).

Primer 17 (SEQ ID NO:35) CTACTCATccatggCATCTTGAGCTTGAGAAAAACC Primer 18 (SEQ ID NO:36) CATCTTACTgcggccgcTTAATGGCTAATCGCCATCTTC

The underlined bases of Primer 17 (forward primer) hybridize to nt 286-307 of the GenBank accession number X03453 sequence which is ˜200 bp upstream from the Cre start codon, while the lower case letters correspond to an NcoI site that was added to the 5′ end of the primer. The underlined bases of Primer 18 (reverse primer) bind at the other end of the Cre open reading frame to nt 1523-1503 of the GenBank accession number X03453 sequence, while the lower case letters indicate a NotI site that was added to the 5′ end of this primer. The 1238 bp PCR product was double-digested with NcoI and NotI, and the resulting DNA fragment, which contains the complete open reading frame for Cre Recombinase and its putative promoters (Sternberg et al., 1986 supra), was purified by agarose gel electrophoresis. The Cre-expression cassette was then inserted between the NcoI and NotI sites of the pZB188/Kan DNA fragment that was described above in a standard ligation reaction. An aliquot of the ligation reaction mixture was electroporated into E. coli DH10B, and the transformed cells were plated on LB media that contained kanamycin (50 μg/ml); growth was at 37° C. Plasmid DNA was isolated from one of the kanamycin-resistant transformants, and this preparation was then introduced into E. coli JM110 (dcm⁻¹, dam⁻) to obtain non-methylated plasmid DNA for subsequent transformation of Z. mobilis (see below). A plasmid map of the Cre Expression vector pZB188/Kan-Cre is shown in FIG. 22.

Cre Treatment to Remove the Selectable Marker from the Chromosome of ZW800 and Curing of the Cre Expression Vector

The Cre Recombinase of bacteriophage P1 (Cre) is able to recognize a specific 34-bp DNA sequence, a “loxP site”, which contains two 13-bp inverted repeats that flank an 8-bp asymmetric core (Sternberg and Hamilton, 1981 supra; Lee and Saito, supra; Trinh et al. supra). Cre is also able to excise any intervening DNA fragment that is situated between two identical loxP sites, and the excision reaction is very rapid. To remove the Spec^(r)-cassette from the GFOR open reading frame, the Cre Expression vector (pZB188/Kan-Cre) was introduced into ZW800. The transformation protocol was essentially as described in Example 5, but after the recovery period the cells were plated on MMG media that contained 350 mg/ml of kanamycin, which is the selective agent for the Cre Expression vector. The primary transformants that were recovered from this process were no longer resistant to spectinomycin, since the Spec^(r)-cassette that was removed from the chromosome by Cre is a circular piece of DNA that cannot replicate in Z. mobilis. After a 48-hr incubation period at 30° C. under anaerobic conditions, two of the Kan^(r)/Spec^(s) primary transformants were subjected to the Cre plasmid-curing process. Although pZB188/Kan-Cre can replicate in Z. mobilis it is relatively easy to cure this plasmid by growing the cells in media that does not contain kanamycin. To cure the Cre Expression vector in the present invention, the cells were grown at an elevated temperature (37° C.) in liquid MMG media that did not contain kanamycin; the cells were transferred to fresh growth media with the same composition every 24-36 hours. After at least 50 generations had occurred, single colonies were isolated on MMG plates, and five colonies from both of the original primary transformants were randomly selected for further characterization. As anticipated, none of these colonies were able to grow on MMG plates that contained kanamycin (350 μg/ml) or spectinomycin (200 μg/ml). Although the inability to grow on kanamycin was a good indication that the plasmid-curing process was successful, this conclusion was confirmed by colony PCR using primers that hybridize to the Cre-expression cassette. Based on these experiments, three of the Cre-treated, plasmid-cured ZW800 derivatives were selected for further characterization and these strains are referred to below as ZW801-4, ZW801-5 and ZW801-6.

To see how well these strains perform in a concentrated mixture of glucose and xylose in the presence of an inhibitory concentration of acetate, shake flask experiments were performed. ZW658 and ZW800 were also included in this analysis. The seed cultures were grown at 30° C. to an OD₆₀₀ of ˜3.0 in liquid media that contained 75 g/L glucose, 25 g/L xylose, 10 g/L yeast extract, 2 g/L KH₂PO₄, 1 g/L MgSO₄, and a 10% inoculum was used for the 15-ml experimental cultures. The latter were grown in 50-ml test tubes at 30° C. with gentle agitation (150 rpm). The growth media contained 10 g/L yeast extract, 2 g/L KH₂PO₄, 1 g/L MgSO₄, 5 mM sorbitol, 40 mM KHCO₃, 95 g/L glucose, 90 g/L xylose, and 7.7 g/L acetate; the initial pH was adjusted to 5.8 with concentrated phosphoric acid. At various times, aliquots of the cultures were removed for HPLC analysis of the fermentation broth as previously described in Example 6. The compounds of interest for this experiment were glucose, xylose, ethanol and xylitol, and all values are reported in g/L.

As shown in Table 5, ZW658 produced 66.35 g/L of ethanol and left behind 40.6 g/L of residual xylose. ZW658 also produced 3.19 g/L of the unwanted by-product xylitol since it has a functional GFOR enzyme. Similar to what was previously observed in other side-by-side experiments, ZW800 consumed 17% more xylose and produced 6.2% more ethanol than ZW658, and it did not produce any detectable xylitol. Although slightly better results were obtained with ZW801-4 and ZW801-6, these differences are probably within experimental error and are not statistically significant. The relatively poor performance of ZW801-5 that was observed in this experiment is not understood and was not further investigated. Based on these results, strain ZW801-4 was selected for further analysis.

TABLE 5 Shake Flask Experiments with ZW658, ZW800, ZW801-4, ZW801-4, and ZW801-5 in High Sugar Plus Acetate Strain Hours Glucose Xylose Xylitol Ethanol ZW658 0 95.7 89.3 0 3.2 ZW658 15.5 27.75 80.93 0 37.39 ZW658 38 0 42.71 1.85 66.53 ZW658 62 0 40.6 3.19 66.35 ZW800 0 95.7 89.3 0 3.2 ZW800 15.5 30.64 81.36 0 36.05 ZW800 38 0 37.29 0 69.82 ZW800 62 0 32.34 0 70.47 ZW801-4 0 95.7 89.3 0 3.2 ZW801-4 15.5 28.04 80.82 0 37.75 ZW801-4 38 0 36.13 0 70.54 ZW801-4 62 0 30.28 0 71.25 ZW801-5 0 95.7 89.3 0 3.2 ZW801-5 15.5 55.61 85.62 0 21.86 ZW801-5 38 0 46.83 0 64.92 ZW801-5 62 0 39.54 0 66.19 ZW801-6 0 95.7 89.3 0 3.2 ZW801-6 15.5 32.34 82.02 0 34.89 ZW801-6 38 0 36.39 0 70.64 ZW801-6 62 0 29.55 0 71.74

To confirm the results from the shake flask experiments that suggested that ZW801-4 performed at least as well as ZW800, these two strains were compared under pH-controlled conditions. The seed cultures were grown at 30° C. in media that contained 75 g/L glucose, 25 g/L xylose, 10 g/L yeast extract, 2 g/L KH₂PO₄, 1 g/L MgSO₄. When the OD₆₀₀ reached ˜4.6, 17-ml aliquots of the seed cultures were used to inoculate the pH-controlled bioreactors that contained 153 ml of growth medium. The final 170 ml cultures contained 105 g/L glucose, 100 g/L xylose, 10 g/L yeast extract, 2 g/L KH₂PO₄, 1 g/L MgSO₄, 5 mM sorbitol and 7.2 g/L of acetate. Growth was at 33° C. and pH was maintained at 5.5 by automated addition of 4 N KOH; the mixing speed was ˜150 rpm. At various times, aliquots of the cultures were removed from the bioreactors for HPLC analysis of the fermentation broth as described above, and OD₆₀₀ was also monitored. Under these experimental conditions, the growth curves for ZW800 and ZW801-4 were almost superimposable (FIG. 23A). The time courses for glucose and xylose consumption were also virtually identical, and both strains produced the same amount of ethanol with similar kinetics (FIG. 23B). Furthermore, neither of these strains produced any detectable xylitol. Based on these observations, we conclude that removing the Spec^(r)-cassette from the GFOR open reading frame did not restore or partially restore GFOR enzyme activity, and that this manipulation did not adversely effect fermentation performance. Although ZW800 and ZW801-4 both performed better than the parent strain (ZW658), which has a functional GFOR enzyme, the preferred strain for commercial applications is ZW801-4 since it does not contain a foreign gene that confers resistance to an antibiotic.

Sequence analysis of genomic DNA from ZW801-4 provided unequivocal proof that the correct Cre excision event had indeed occurred. The complete nucleotide sequence of the disrupted GFOR open reading in ZW801-4 (from the original start codon through the original stop codon) is given in SEQ ID NO:37, and FIG. 24 shows an alignment of the translated mutant sequence with the wild type GFOR protein; the latter is coded for by the reverse complement of nt 683751-685052 of GenBank accession number AE008692. As anticipated, Cre excision of the Spec^(r)-cassette left a single wild type loxP site in the middle of the GFOR open reading frame, and this insertion event resulted in an in-frame stop codon that prematurely truncates the protein; the location of the “lox scar” is indicated by the gray highlighted residues. The mutant nucleotide sequence is also missing ˜72 bp of the original wild type GFOR nucleotide sequence in the same location as a result of the design of the suicide construct. 

1. A process for producing ethanol comprising, a) providing a recombinant Zymomonas strain which utilizes xylose to produce ethanol., said strain comprising at least one genetic modification which reduces glucose-fructose oxidoreductase activity, and b) culturing the strain of (a) in a medium comprising xylose whereby xylose is converted to ethanol.
 2. The process according to claim 1, wherein the strain of (a) improves conversion of xylose to ethanol relative to a recombinant Zymomonas strain without at least one genetic modification which reduces glucose-fructose oxidoreductase activity.
 3. The process of claim 2, wherein the strain of (a) improves one or more of rate, titer or yield, of xylose conversion to ethanol relative to a recombinant Zymomonas strain without at least one genetic modification which reduces glucose-fructose oxidoreductase activity.
 4. The process according to claim 1, wherein the strain of (a) produces a reduced amount of xylitol when metabolizing xylose to ethanol as compared to a Zymomonas strain without at least one genetic modification which reduces glucose-fructose oxidoreductase activity.
 5. The process according to claim 4, wherein the strain of (a) produces substantially no xylitol when metabolizing xylose to ethanol.
 6. The process according to claim 1, wherein the recombinant Zymomonas strain of (a) is selected from the group consisting of ZW800, ZW801-4 and ZW801-6.
 7. The process of claim 1, wherein the medium comprises a mixture of sugars including xylose and a sugar alcohol selected from the group consisting of sorbitol, mannitol, galactitol, ribitol, and a mixture thereof, wherein the mixture of sugars is at a concentration of at least about 120 g/L and wherein the sugar alcohol is at a final concentration that is between about 2 mM and about 100 mM.
 8. The process of claim 7, wherein the sugar alcohol is in a concentration that is between about 5 mM and about 20 mM. 